Altering the interface of hydrocarbon-coated surfaces

ABSTRACT

Methods and compositions are provided wherein microorganisms are used to alter the interface of hydrocarbons and hydrocarbon-coated surfaces to increase oil recovery, for improved bioremediation and/or pipeline maintenance.

This application claims the benefit of U.S. Provisional Applications 61/180,529, field May 22, 2009 and 61/180,445, filed May 22, 2009 and U.S. National Application Ser. No. 12/784,518, filed May 21, 2010.

FIELD OF INVENTION

This invention relates to the field of environmental microbiology and modification of heavy crude oil properties using microorganisms. More specifically, microorganisms are used to alter the interface between hydrocarbons and a surface to increase oil recovery, from hydrocarbon coated surfaces.

BACKGROUND OF THE INVENTION

Hydrocarbons in the form of petroleum deposits and oil reservoirs are distributed worldwide. These oil reservoirs are measured in the hundreds of billions of recoverable barrels. Because heavy crude oil has a relatively high viscosity and may adhere to surfaces, it is essentially immobile and cannot be easily recovered by conventional primary and secondary means.

Microbial Enhanced Oil Recovery (MEOR) is a methodology for increasing oil recovery by the action of microorganisms (Brown, L. R., Vadie, A. A, Stephen, O. J. SPE 59306, SPE/DOE Improved Oil Recovery Symposium, Oklahoma, Apr. 3-5, 2000). MEOR research and development is an ongoing effort directed at discovering techniques to use microorganisms to benefit oil recovery (Sunde. E., Beeder, J., Nilsen, R. K. Torsvik, T., SPE 24204, SPE/DOE 8th Symposium on enhanced Oil Recovery, Tulsa, Okla., USA, Apr. 22-24, 1992). An effective MEOR treatment for crude oil desorption and mobilization could utilize microbially derived surface active agents (McInerney, M. J., et al., Development of microorganisms with improved transport and biosurfactant activity for enhanced oil recovery. DE-FE-02NT15321. DOE, 2003). Few have been identified that have been shown to alter the surface interaction between hydrocarbons and rocks, soil, brine, sand or clay to which the hydrocarbons are adhered.

Use of surface active agents or surfactants to increase solubility of oil through reduction in surface and interfacial tensions is another technique for increasing oil recovery. A wide variety of surfactants identified thus far are able to significantly reduce surface and interfacial tensions at the oil/water and air/water interfaces. Because surfactants partition at oil/water interfaces, they are capable of increasing the solubility and bioavailability of hydrocarbons (Desai, J. D. and I. M. Banat. Microbial production of surfactants and their commercial potential. Microbiol. Mol. Biol. Rev., 47-64, 1997 and Banat, I. M. Bioresource Technol. 51: 1-12, 1995 and Kukukina, M. S., et al. Environment International. 31: 155-161, 2005 and Mulligan, C., Environmental Pollution. 133: 183-198, 2005). Doong and Lei (J. Hazardous Materials. B96: 15-27, 2003), for example, found that the addition of surfactants to soil environments contaminated with polyaromatic hydrocarbons increased the mineralization rate of some hydrocarbons (Doong, R and W. Lei, supra). Such surfactants are expensive and may pose environmental or other equipment issues.

Biosurfactants, (biologically produced surfactants), have helped to substantially increase oil recovery from sandstone deposits by increasing solubility and decreasing viscosity of the oil (Mulligan, C., supra). Depending on the application, biosurfactants may be preferred since they are generally more biodegradable and less toxic than synthetically produced surfactants, and are effective under a broad range of oil and reservoir conditions. Examples of biosurfactants include glycolipids, lipopeptides and lipoproteins, fatty acids and phospholipids, polymeric compounds, and particulate biosurfactants (Desai, J. D. supra). However, further characterization of production and use of biosurfactants is needed. Further, there is a need to identify microorganisms that are able to produce these biosurfactants under reservoir conditions or other relevant environmental conditions.

Certain microorganisms have been described as having properties that may benefit MEOR processes. Certain Shewanella species have been disclosed as useful for remediation of metal contamination (U.S. Pat. No. 6,923,914B2), iron containing mixed waste (U.S. Pat. No. 6,719,902B1), manganese contamination (U.S. Pat. No. 6,350,605B1), and other pollutants with the aide of butane (U.S. Pat. No. 6,245,235B1). In EP1189843, certain Shewanella species were described as being useful for bioremediation of petroleum contaminants aerobically. In addition, Shewanella supplemented with butane was used for reduction of fouling in injection and recovery wells under aerobic conditions (U.S. Pat. No. 6,244,346B1). Other Shewanella species have been described as having the ability to produce biofilms (D. Bagge, et al., Appl. Environ. Microbiol. 67, 2319-2325. 2001); to sequester gases, in particular CO₂, in underground geological formations and prevent their release into the atmosphere (see US20060216811A1); and to enhance oil recovery (commonly owned and co-pending US 2009-0260803 A1). The activity reported by these microorganisms is related to the degradation and transformation of hydrocarbons and other pollutants and not related to altering the interfacial boundaries between hydrocarbons and the surfaces to which they are bound.

The problem to be solved therefore, relates to the identification of microorganisms that: 1) have the ability to alter the interface between hydrocarbons and rock or other surfaces subject to coating by oil; 2) can be inoculated under suitable conditions which effect these alterations in surface properties; and 3) can be used in a cost-efficient way, to improve oil recovery, and benefit bioremediation.

SUMMARY OF THE INVENTION

The methods described herein solve the stated problem above, by identifying microorganisms that have the ability to alter the interface between hydrocarbons and the surfaces which they coat in order to improve oil recovery, and benefit bioremediation. The alterations result in substantial liberation of oil from hydrocarbon-coated surfaces. In one aspect the microorganisms are Shewanella, species that have the ability to affect the wettability of the surfaces through microbial action. In addition, a new isolate of Shewanella sp. has been identified.

-   -   Accordingly invention provides a method for altering the         wettability of a hydrocarbon coated surface comprising:         -   a) providing a hydrocarbon-coated surface;         -   b) providing a medium selected from the group consisting of:             -   i) a cell containing medium comprising one or more                 Shewanella sp.; and             -   ii) a conditioned medium which is substantially cell                 free and which has been in contact with one or more                 Shewanella sp.;         -   c) contacting said hydrocarbon-coated surface with the             medium of b) wherein the medium alters the wettability of             said hydrocarbon-coated surface.     -   In another aspect of the invention the invention provides a         method for oil recovery from an oil reservoir comprising:         -   a) providing one or more Shewanella sp;         -   b) injecting an oil reservoir with the one or more             Shewanella sp of (a); and         -   c) injecting said oil reservoir with a nutrient solution             comprising one or more electron acceptors selected from the             group consisting of nitrate, fumarate, ferric ion, manganese             (MnIV) ion and mixtures thereof;     -   wherein said one or more Shewanella sp. grow under anaerobic         conditions in the oil reservoir and said growth promotes         improved oil recovery.

In another aspect of the invention the invention provides a composition for enhanced oil recovery comprising:

-   -   a) a Shewanella sp having a 16S rDNA that has at least 95%         identity to the 16S rDNA sequence as set forth in any of SEQ ID         NO.'s 3, 5, 15, 16 and 17; and     -   b) an electron acceptor selected from the group consisting of         nitrate, fumarate, ferric ion, manganese (MnIV) ion and mixtures         thereof.         In another aspect of the invention the invention provides a         Shewanella sp. having the following characteristics:     -   a) a 16S rDNA comprising signature sequences SEQ ID NOs: 13 and         14; and     -   b) riboprint pattern identifier of 212-824-S-4 as illustrated in         FIG. 16;

wherein 16S rDNA of (a) has at least about 97% identity to the 16S rDNA sequence as set forth in SEQ ID NO:3.

BRIEF DESCRIPTION OF FIGURES AND SEQUENCES OF THE INVENTION

The invention can be more fully understood from the following detailed description, the Figures, and the accompanying sequence descriptions, which form a part of this application.

FIG. 1 shows the relative sand release by strain LH4:18 cultures over a period of three weeks. After about 6 days, a 6 mm zone of released sand was observed in the bottom of the wells for the week old (week 1—solid line) culture and a 3 mm zone was observed for the day-old sample (Day 1—dotted line).

FIG. 2 depicts sand/oil release using either an aerobic or an anaerobic culture. PPGAS medium samples (PPGAS), with and without supplements, were used as controls in both aerobic and anaerobic experiments. The Shewanella strain (LH4:18) was used in the experiment. Experiments were performed in the absence of lactate and nitrate (L/N) or in their presence in both anaerobic and aerobic experiments.

FIG. 3 depicts a comparison of CFU/mL in various samples, expressed as Log 10 (MPN), on the day of the LOOS test set up (Day 3) and the relative sand release for each sample. The symbols designate presence of the following ingredients in the growth medium: fumarate (F); nitrate (N); and lactate and nitrate (L/N).

FIG. 4 depicts sand/oil release by Shewanella strain (LH4:18) in the presence or absence of glucose. One week old cultures were used and the experiment was continued for 20 days. One set of cultures did not receive any glucose and another set received 0.5% glucose. The experiment was performed for one week in the absence of any heat.

FIG. 5 depicts oil release over time with strain LH4:18 grown in the presence of different media and supplements for 21 days. Where indicated, supplements were 1% peptone, 1.6 mM MgSO₄, 20 mM KCl, 20 mM NH₄Cl, and 20 mM tris base.

FIG. 6 shows the ability of Shewanella strain (LH4:18) to release oil in sand/oil release was tested for 13 days using the SIB medium either with peptone or YE added. The controls contained medium but no microbes.

FIG. 7 shows sand/oil release using either cell free supernatants of the Shewanella strain (LH4:18) cultures or the whole culture. The experiment was performed for 19 days.

FIG. 8 depicts oil release over time with strain LH4:18 cell free supernatant (centrifuged compared with centrifuged and filtered) and strain LH4:18 cell pellet resuspended in fresh medium.

FIG. 9 depicts the results of the ability of strain LH4:18 to release sand/oil in the presence of other organisms such as Pseudomonas stutzeri strain LH4:15. One set of the experiment was performed measuring sand/oil release by LH4:15, another set used strain LH4:18 and the third set used a mixture of both LH4:15 and LH4:18. The experiment was performed for 21 days.

FIG. 10 depicts oil release over time with LH4:18 and other Shewanella species (strains EH60:12, EH60:2, and EH60:10). The experiment was performed for 19 days.

FIG. 11 depicts oil release over time in a LOOS test in the presence of fumarate or nitrate as the electron acceptors. The experiment was performed for 14 days with LH4:18 and other Shewanella species purchased through DSMZ (Deutsche Sammlung von Mikrorganismen and Zellkulturen, German Collection of Microorganisms and Cell Cultures).

FIG. 12 shows photomicrographs of untreated oil coated sand (FIG. 12A) compared to oil coated sand treated with Shewanella LH4:18 (FIG. 12B). The lines drawn on the picture depict the contact angle between the hydrocarbon and the sand through the oil.

FIG. 13 depicts the level of average residual oil saturation along the sand pack column. The results with control are shown with diamonds and the results with the inoculated (strain LH4:18) are shown with squares. The amount of residual oil saturation in the control column was 22.5% whereas the residual oil saturation for strain LH4:18 inoculated columns was 16.1%, indicating that strain LH4:18 was able to reduce residual oil saturation by approximately 6.5%.

FIG. 14 shows strain and species-specific signature base variations that occur in strain L3:3 in the 16S rRNA variable region 3 and SEQ ID NO: 13 (bp coordinates 430 to 500) at specific coordinate positions: 438-40, 451, 454-57, 466-69, 471, 484-86 and 496.

FIG. 15 shows strain and species-specific signature base variations for bacterial variable region 6 for sequences closely related to Shewanella sp L3:3, e.g., sequences similar to that defined by SEQ ID NO: 14. Strain and species-specific variations occur between base coordinates 990 and 1049, specifically at positions: 995-6, 1001-5, 1007, 1012, 1014, 1016-18 and 1035.

FIG. 16 shows the Riboprint batch report, 052009, used for comparisons of Shewanella sp. L3:3 designated riboprint #212-824-S-4 to other Shewanella riboprints available in the Qualicon and DuPont Environmental Sciences Riboprint Databases.

FIG. 17 shows the a typical image of untreated oil coated sand (FIG. 17A) with a low contact angle through the oil (qCA—FIG. 17B) and the effect of exposure of the oil coated sand to strain L3:3 (FIG. 17C) which shows a significant increase in the contact angle through the oil on the oil coated sand (qCB—FIG. 17D).

FIG. 18 shows dominant and degenerate signature sequences for Shewanella species in rDNA variable regions 2 (A), 5 (B), and 8 (C). The variable positions are underlined. Alternative nucleotides for each variable position designation are given in the legend. Shewanella oneidensis MR-1 is representative of Shewanella having the dominant signature sequences.

The following DNA sequences conform with 37 C.F.R. 1.821-1.825 (“Requirements for Patent Applications Containing Nucleotide Sequences and/or Amino Acid Sequence Disclosures—the Sequence Rules”) and are consistent with World Intellectual Property Organization (WIPO) Standard ST.25 (1998) and the sequence listing requirements of the EPO and PCT (Rules 5.2 and 49.5(a-bis), and Section 208 and Annex C of the Administrative Instructions. The symbols and format used for nucleotide and amino acid sequence data comply with the rules set forth in 37 C.F.R. §1.822.

SEQ ID NO:1 is oligonucleotide primer 1492R.

SEQ ID NO:2 is oligonucleotide primer 8F.

SEQ ID NO:3 is 16S rDNA from Shewanella sp. L3:3

SEQ ID NO:4 is 16S rDNA from CP000681 Shewanella putrefaciens CN-32.

SEQ ID NO:5 is 16S rDNA from Shewanella putrefaciens LH4:18.

SEQ ID NO:6 is 16S rDNA FJ210800 from Shewanella algae.

SEQ ID NO:7 is 16S rDNA EU563337.1 from Shewanella sp. C13-M.

SEQ ID NO:8 is 16S rDNA EU563345.1 from Shewanella sp. C31.

SEQ ID NO:9 is 16S rDNA DQ164801.1 from Shewanella sp. L10.

SEQ ID NO:10 is 16S rDNA FM210033.2 from Shewanella chilikensis JC5T.

SEQ ID NO:11 is 16S rDNA EU721813 from Shewanella uncultured clone D004024H07.

SEQ ID NO:12 is 16S rDNA EU563338.1 from Shewanella sp. C16-M.

SEQ ID NO:13 is the DNA sequence corresponding to prokaryote 16S rRNA variable region 3 that is signature to Shewanella sp. L3:3 and related strains.

SEQ ID NO:14 is the DNA sequence corresponding to prokaryote 16S rRNA variable region 6 that is signature to Shewanella sp. L3:3 and related strains.

SEQ ID NO:15 is a partial sequence of the 16S rDNA of Shewanella sp. strain EH60:12.

SEQ ID NO:16 is a partial sequence of the 16S rDNA of Shewanella sp. strain EH60:10.

SEQ ID NO:17 is a partial sequence of the 16S rDNA of Shewanella sp. strain EH60:2.

SEQ ID NO:18 is the Shewanella dominant signature sequence for the 16S rDNA variable region 2.

SEQ ID NO:19 is the Shewanella degenerate signature sequence for the 16S rDNA variable region 2.

SEQ ID NO:20 is the Shewanella dominant signature sequence for the 16S rDNA variable region 5.

SEQ ID NO:21 is the Shewanella degenerate signature sequence for the 16S rDNA variable region 5.

SEQ ID NO:22 is the Shewanella dominant signature sequence for the 16S rDNA variable region 8.

SEQ ID NO:23 is the Shewanella degenerate signature sequence for the 16S rDNA variable region 8.

Applicants have made the following biological deposits under the terms of the Budapest Treaty on the International Recognition of the Deposit of Microorganisms for the Purposes of Patent Procedure:

TABLE 1 INFORMATION ON DEPOSITED STRAINS International Depositor Identification Depository Reference Designation Date of Deposit Shewanella sp L3:3 ATCC No. PTA-10980 May 19, 2010 Shewenella putrefaciens ATCC No. PTA-8822 Dec. 4, 2007 LH4:18

DETAILED DESCRIPTION

Applicants specifically incorporate the entire content of all cited references in this disclosure. Unless stated otherwise, all percentages, parts, ratios, etc., are by weight. Trademarks are shown in upper case. Further, when an amount, concentration, or other value or parameter is given as either a range, preferred range or a list of upper preferable values and lower preferable values, this is to be understood as specifically disclosing all ranges formed from any pair of any upper range limit or preferred value and any lower range limit or preferred value, regardless of whether ranges are separately disclosed. Where a range of numerical values is recited herein, unless otherwise stated, the range is intended to include the endpoints thereof, and all integers and fractions within the range. It is not intended that the scope of the invention be limited to the specific values recited when defining a range.

The invention relates to methods for altering the interfacial properties of hydrocarbon coated surfaces by contacting these surfaces with Shewanella microorganisms that have the ability to alter the interface between the hydrocarbons and such surfaces. These alterations result in substantial oil liberation from the hydrocarbon-coated surfaces. It has been discovered that these Shewanella sp. have the ability to affect the wettability of the surfaces through microbial action and thereby provide for increased oil recovery form those surfaces. Wettability may also be altered by media conditioned by growth of said microorganisms.

In addition, the invention relates to the identification of previously unknown Shewanella sp. isolated from production water samples obtained from an oil reservoir.

The following definitions are provided for the special terms and abbreviations used in this application:

The abbreviation “dNTPs” refers to Deoxyribonucleotide triphosphates.

The abbreviation “ATCC” refers to American Type Culture Collection International Depository, Manassas, Va., USA. “ATCC No.” refers to the accession number to cultures on deposit with ATCC.

The abbreviation “ASTM” refers to the American Society for Testing and Materials.

The term “terrestrial subsurface formation” or “subsurface formation” refers to in ground or underground geological formations and may comprise elements such as rock, soil, brine, sand, shale, clays and mixtures thereof.

The term “terrestrial surface formation” or “surface formation” refers to above ground geological formations and may comprise elements such as rock, soil, brine, sand, shale, clays and mixtures thereof.

The term “environmental sample” means any sample exposed to hydrocarbons, including a mixture of water and oil. As used herein environmental samples include water and oil samples that comprise indigenous microorganisms useful for phylogenetic mapping of genera present in a given sampling area.

The term “environmental site” means a site that has been contaminated with hydrocarbons and/or other persistent environmental pollutants. Environmental sites may be in surface or subsurface locations.

“Production wells” are wells through which oil is withdrawn from a reservoir. An oil reservoir or oil formation is a subsurface body of rock having sufficient porosity and permeability to store and transmit oil.

The term “sweep efficiency” means the ability of injected water to ‘push’ oil through a geological formation toward a producer well. One problem that can be encountered with waterflooding operations is the relatively poor sweep efficiency of the water, i.e., the water can channel through certain portions of the reservoir as it travels from the injection well(s) to the production well(s), thereby bypassing other portions of the reservoir. Poor sweep efficiency may be due, for example, to differences in the mobility of the water versus that of the oil, and permeability variations within the reservoir which encourage flow through some portions of the reservoir and not others.

The term “irreducible water saturation” is the minimal water saturation that can be achieved in a porous core plug when flooding with oil to saturation. It represents the interstitial water content of the matrix where the water is never completely displaced by the oil because a minimal amount of water must be retained to satisfy capillary forces.

The term “growing on oil” means the microbial species are capable of metabolizing hydrocarbons or other organic components of crude petroleum as a nutrient to support growth.

The term “remediation” refers to the process used to remove hydrocarbon contaminants from an environmental site containing hydrocarbons and/or other persistent environmental pollutants.

The term “bioremediation” refers to the use of microorganisms to remediate or detoxify contaminants form a contaminant-altered environment

“Petroleum” or “oil” is a naturally occurring, flammable liquid found in rock and sand formations in the Earth, which consisting of a complex mixture of hydrocarbons and polycyclic aromatic hydrocarbon of various molecular weights, plus other organic compounds.

“Crude oil” refers to the unrefined oil taken from a petroleum reservoir.

“Oil well” and “oil reservoir” may be used herein interchangeably and refer to a subsurface formation from which oil may be recovered.

“Interface” as used herein refers to the surface of contact or boundary between immiscible materials, such as oil and water or a liquid and a solid. As used herein “interfaces” may be between a water layer and an oil layer, a water layer and a solid surface layer, or an oil layer and a solid surface layer.

“Hydrocarbon-coated” as used herein refers to a coating of a hydrocarbon to a solid surface of at least 10% areal coverage.

The term “components of a subsurface formation” refers to rock, soil, brine, sand, shale, clay or mixtures thereof of either subterranean or seabed formations, that have come in contact with one or more hydrocarbon. These components may be part of an oil well or reservoir. At least a portion of the components include some hydrocarbon-coated surfaces, including particles with coated surfaces.

“Adhered to” refers to coating or adsorption of a liquid to a solid surface of at least 10% areal coverage.

“Shewanella species” or “Shewanella sp.” is a bacterial genus that has been established, in part through phylogenetic classification by rDNA. There is at least about 89% sequence identity of 16S rDNA sequences among Shewanella species. The 16S rDNA sequences of Shewanella species have at least about 89% sequence identity to any of SEQ ID NOs:3-12. Shewanella species have 16S rDNA which has the signature sequences of regions 2 (SEQ ID NO:18, 19), 5, (SEQ ID NO:20,21) and 8 (SEQ ID NO: 22,23) as shown in FIG. 18. The degenerate signature sequence for each region gives the sequence that defines Shewanella species, including some position variations as shown in FIG. 18. The dominant signature sequences in FIG. 18 are those with the variable positions designated as the most frequently found nucleotides in Shewanella species. Shewanella are gram negative, gamma-proteobacteria, which have the ability to reduce metals and are capable of additionally reducing a wide range of terminal electron acceptors. These microorganisms gain energy to support anaerobic growth by coupling the oxidation of H₂ or organic matter to the redox transformation of a variety of multivalent metals, which leads to the precipitation, transformation, or dissolution of minerals.

The abbreviation “rDNA” refers to ribosomal deoxyribonucleic acid gene sequence.

The term “rDNA typing” means the process of using the sequence of the 16S rDNA gene to obtain the “closest relative” microbial species by homology to rDNA sequences maintained in several international databases.

The term “phylogenetic typing” “phylogenetic mapping” or “phylogenetic classification” may be used interchangeably herein and refer to a form of classification in which microorganisms are grouped according to their ancestral lineage. The methods herein are specifically directed to phylogenetic typing on environmental samples based on 16S Ribosomal DNA (rDNA) sequencing. In this context, approximately 1400 base pair (bp) length of the 16S rDNA gene sequence is generated using 16S rDNA universal primers identified herein and compared by sequence homology to a database of microbial rDNA sequences. This comparison is then used to help taxonomically classify pure cultures for use in enhanced oil recovery.

The term “ribotyping” or “riboprint” refers to fingerprinting of genomic DNA restriction fragments that contain all or part of the rRNA operon encoding for the 5S, 16S and 23S rRNA genes (Webster, John A, 1988. U.S. Pat. No. 4,717,653; Bruce, J. L., Food Techno., (1996), 50: 77-81; and Sethi, M. R., Am. Lab. (1997), 5: 31-35). Ribotyping, involves generation of restriction fragments, from microbial chromosomal DNA, which are then separated by electrophoresis, and transferred to a filter membrane and finally probed with labeled rDNA operon probes. Restriction fragments that hybridize to the labeled probe produce a distinct labeled pattern or fingerprint/barcode that is unique to a specific microbial strain. The “riboprint” is a unique fingerprint pattern that can be given a unique riboprint identifier” (alphanumeric characters) and stored electronically to be used to identify the isolate when compared to the database at a later date. The ribotyping procedure can be entirely performed on the Riboprinter® instrument (DuPont Qualicon, Wilmington, Del.).

The term “riboprint batch” refers to comparison alignment of two or more riboprints and is depicted in a report as a pictograph.

The term “percent identity”, as known in the art, is a relationship between two or more polypeptide sequences or two or more polynucleotide sequences, as determined by sequence comparisons. In the art, “identity” also means the degree of sequence relatedness or homology between polynucleotide sequences, as determined by the match between strings of such sequences and their degree of invariance. The term “similarity” refers to how related one nucleotide or protein sequence is to another. The extent of similarity between two sequences is based on the percent of sequence identity and/or conservation. “identity” and “similarity” can be readily calculated by known methods, including but not limited to those described in “Computational Molecular Biology, Lesk, A. M., ed. Oxford University Press, NY, 1988”; and “Biocomputing: Informatics and Genome Projects, Smith, D. W., ed., Academic Press, NY, 1993”; and “Computer Analysis of Sequence Data, Part I, Griffin, A. M., and Griffin, H. G., eds., Humana Press, NJ, 1994”; and “Sequence Analysis in Molecular Biology, von Heinje, G., ed., Academic Press, 1987”; and “Sequence Analysis Primer, Gribskov, M. and Devereux, J., eds., Stockton Press, NY, 1991”. Preferred methods to determine identity are designed to give the best match between the sequences tested. Methods to determine identity and similarity are codified in publicly available computer programs such as sequence analysis software. Typical sequence analysis software includes, but is not limited to: the GCG suite of programs (Wisconsin Package Version 9.0, Genetics Computer Group (GCG), Madison, Wis.), BLASTP, BLASTN, BLASTX (Altschul et al., J. Mol. Biol. 215, 403-410,1990), DNASTAR (DNASTAR, Inc., Madison, Wis.), and the FASTA program incorporating the Smith-Waterman algorithm (Pearson, W. R., Comput. Methods Genome Res., Proc. Int. Symp, Meeting Date 1992, 111-120, Eds: Suhai, Sandor, Plenum Publishing, New York, N.Y., 1994). Within the context of this application, it will be understood that, where sequence analysis software is used for analysis, the results of the analysis will be based on the “default values” of the program referenced, unless otherwise specified. As used herein “default values” will mean any set of values or parameters which originally load with the software when first initialized. The term “wetting” refers to the ability of a liquid to maintain contact with a solid surface, resulting from intermolecular interactions when the two are brought together. The degree of wetting (expressed as “wettability”) is determined by a force balance between adhesive and cohesive forces.

“Wetting agent” refers to a chemical such as a surfactant that increases the water wettability of a solid or porous surface by changing the hydrophobic surface into one that is more hydrophilic. Wetting agents help spread the wetting phase (e.g., water) onto the surface thereby making the surface more water wet.

“Wettability” refers to the preference of a solid to contact one liquid, known as the wetting phase, rather than another. Solid surfaces can be water wet, oil wet or intermediate wet. “Water wettability” pertains to the adhesion of water to the surface of a solid. In water-wet conditions, a thin film of water coats the solid surface, a condition that is desirable for efficient oil transport.

The term “adhesive forces” refers to the forces between a liquid and solid that cause a liquid drop to spread across the surface. The “cohesive forces” refers to forces within the liquid that cause the drop to ball up and avoid contact with the surface.

The term “contact angle” is the angle at which a liquid (oil or water) interface meets a solid surface, such as sand or clay. Contact angle is a quantitative measurement of the wetting of a solid by a liquid and is specific for any given system, and is determined by interactions across three interfaces. The concept is illustrated with a small liquid droplet resting on a flat horizontal solid surface. The shape of the droplet is determined by the “Young Relation” (Bico et al., Colloids and Surfaces A: Physicochemical and Engineering Aspects 206 (2002) 41-46). The theoretical description of contact arises from the consideration of a thermodynamic equilibrium between the three phases: the liquid phase of the droplet (L), the solid phase of the substrate (S), and the gas/vapor phase of the ambient (V) (which will be a mixture of ambient atmosphere and an equilibrium concentration of the liquid vapor). The V phase could also be another (immiscible) liquid phase. At equilibrium, the chemical potential in the three phases should be equal. It is convenient to frame the discussion in terms of interfacial energies. The solid-vapor interfacial energy (see surface energy) is γ_(SV), the solid-liquid interfacial energy is γ_(SL) and the liquid-vapor energy (i.e. the surface tension) is simply γ. The Young equation: 0=γ_(SV)−γ_(SL)-cos θ is written such that describes an equilibrium where θ_(C) is the equilibrium contact angle.

“Microbial populations” means one or more populations of microorganisms present, either in samples obtained from oil wells or in an inoculum for injection into an oil well or subsurface formation.

“Medium” as used herein means an aqueous milieu either comprises one of more Shewanella sp. or is a cell free supernatant that has been in contact with one or more Shewanella sp. Medium containing Shewanella sp. is referred to herein as “cell containing” medium and medium that is a cell free supernatant is referred to herein as “cell free” medium. Medium will be aqueous based any may contain various nutrients, buffers, salts, vitamins, co-factors and the like and carbon sources useful for microbial growth.

“Electron acceptor” is a molecular compound that receives or accepts an electron during cellular respiration. Microorganisms obtain energy to grow by transferring electrons from an “electron donor” to an electron acceptor. During this process, the electron acceptor is reduced and the electron donor is oxidized. Examples of acceptors include oxygen, nitrate, fumarate, iron (III), manganese (IV), sulfate or carbon dioxide. Sugars, low molecular weight organic acids, carbohydrates, fatty acids, hydrogen and crude oil or its components such as petroleum hydrocarbons or polycyclic aromatic hydrocarbons are examples of compounds that can act as electron donors.

“Denitrifying” and “denitrification” mean reducing nitrate for use as an electron acceptor in respiratory energy generation. “Denitrifying conditions” means conditions where denitrification occurs.

“Inoculating an oil well” means injecting one or more microorganisms or microbial populations or a consortium into an oil well or oil reservoir such that microorganisms are delivered to the well or reservoir without loss of total viability. The term “simple nitrates” and “simple nitrites” refer to nitrite (NO₂) and nitrate (NO₃).

The term “nutrient supplementation” refers to the addition of nutrients that benefit the growth of microorganisms that are capable of using crude oil as their main carbon source but grow optimally with other non-hydrocarbon nutrients, i.e., yeast extract, peptone, succinate, lactate, formate, acetate, propionate, glutamate, glycine, lysine, citrate, glucose, pyruvate and vitamin solutions.

The term “biofilm” means a film or “biomass layer” made up of a matrix of a compact mass of microorganisms consisting of structural heterogeneity, genetic diversity, complex community interactions, and an extracellular matrix of polymeric substances. Biofilms are often embedded in these extracellular polymers, which adhere to surfaces submerged in, or subjected to, aquatic environment

The term “bacterial” means belonging to the bacteria. Bacteria are an evolutionary domain or kingdom of microbial species separate from other prokaryotes based on their physiology, morphology and 16S rDNA sequence homologies.

“Microbial species” means distinct microorganisms identified based on their physiology, morphology and phylogenetic characteristics using 16S rDNA sequences. The closest relative microbial species may also be referred to as a “homolog”.

The term “pure culture” means a culture derived from a single cell isolate of a microbial species. The pure cultures specifically referred to herein include those that are publicly available in a depository. Additional pure cultures are identifiable by the methods described herein.

The term “simulated injection brine” or “SIB” is a medium composition containing 198 mM NaCl, 1 mM MgCl₂, 1.8 mM CaCl₂, 1.2 mM KCl, 16 mM NaHCO₃, 0.05 mM SrCl₂, 0.13 mM BaCl₂, 0.14 mM LiCl.

The abbreviation “NCBI” refers to the National Center for Biotechnology Information.

A spectrophotometer is a device for measuring light intensity that can measure intensity as a function of the color, or more specifically, the wavelength of light. In microbiology, the term “optical density” is a unit-less measure of the transmittance of light at a given wavelength that uses an empirical relationship that relates the absorption of light to the properties of the material through which the light is traveling.

The term “MPN” or “most probable number” is a quantitative measurement of the concentration of microbes in a given medium. It is expressed as CFU/ml (colony forming units/ml), log 10(CFU/ml) or log 10(MPN).

Altering Hydrocarbon-Surface Interface

Provided herein are methods for oil recovery and remediation which rely on altering the wettability of hydrocarbon-coated surfaces. Through altering wettability, the characteristics of the interface between hydrocarbons and a hydrocarbon-coated surface is changed, thereby releasing the hydrocarbons from the surface. For example, this alteration may result in the surface having a preference for binding water as opposed to oil thereby providing for recovery of the oil more readily. Changes in the wettability may be monitored by measuring changes in the contact angle between a hydrocarbon and the surface to which it is adhered. For example, an increase in the contact angle is an indication of a reduction in the surface energy required to bind the oil to the surface (see Example 8). Thus, an aspect of the present invention is the discovery that contact between Shewanella sp. or biomolecules produced by Shewanella sp., and hydrocarbon coated surfaces produces alterations in the wettability properties of the hydrocarbon coated surface such that the surface energy binding the hydrocarbon to the surface is decreased, (as measured by an increase in the contact angle) resulting in the subsequent release of oil.

Hydrocarbon-coated surfaces may be any hard surface (including one or more particle) that is coated or contaminated with hydrocarbons with at least 10% areal coverage by said hydrocarbons. The hydrocarbons may be adhered to said surfaces. Hydrocarbon-coated surfaces may be in subsurface formations, for example in oil reservoirs, and may include rock, soil, brine, sand, clays, shale, and mixtures thereof. In addition, hydrocarbon-coated surfaces may include materials that are not subsurface including rock, clay, soil, sediments, sand, sludge, harbor dredge spoils, sediments, refinery wastes, wastewater, sea water, and mixtures thereof. In addition, hydrocarbon-coated surfaces may include equipment such as pipelines, oil tanks and tankers, and other machinery that may be contaminated with hydrocarbons.

In the present methods, Shewanella sp. alter the wettability of hydrocarbon-coated surfaces. Alteration may be by contact with said microbes or by contact with extracellular molecules produced by said microbes, which may in include one or more wetting agents. The Shewanella sp. under certain conditions undergo modifications in surface-bound or extracellular molecules. Modifications include changes in the composition and/or ratio of the molecules which include but are not limited to cytochromes, flavins, siderophores, membrane vesicles, glycoproteins, glycolipids, lipoproteins, fimbriae, extracellular polymeric substances, polysaccharides, monosaccharides, and lipopolysaccharides. These modifications, in turn, alter the water wettability of a hydrocarbon-coated surface contacted by the altered microbial surfaces.

Conditions for growth that are suitable for Shewanella species to be used in the present methods are determined by the environment of the target hydrocarbon-coated surface, and the conditions for growth of said species in a given environment. Suitable conditions include those that are favorable to producing changes in the wettability of the hydrocarbon-coated surface. Such suitable conditions may include growth and medium compositions that are beneficial for the production and/or modification of surface bound or extracellular molecules, especially those molecules related to stress, oxygen limitation, redox, and/or electron transfer which may be wetting agents. Typical growth media compositions include enriched media containing diverse nutrient sources such as peptone, yeast extract, or casamino acids, for example. In some aspects the medium may be a minimal medium such as SL10 or simulated injection brine supplemented with an electron donor and electron acceptor. Examples of electron donors include, but are not limited to, lactate and/or acetate. Examples of electron acceptors include but are not limited to, nitrate, fumarate, pyruvate, ferric ion (Fe (III)) and/or manganese ion (Mn (IV). Additional carbon sources may include but are not limited to yeast extract, peptone, pyruvate, glucose, succinate, formate, propionate, glutamate, glycine lysine, oil, and oil components. Oil components may be any of the many components that are present in crude oil. Cultures may be grown aerobically or anaerobically, and may be grown at a temperature that is similar to that of a target reservoir, typically about 30° C., or in the range of room temperature, +/−5° C. In addition, stress conditions may be suitable for growth of the present strains. Growth under stress inducing conditions includes, but is not limited to, switching growth from oxic to anoxic conditions, growth under population pressure or high density growth, switching electron acceptors, growth at low temperatures, and growth under osmotic stress (such as in high salt).

Cultures of Shewanella species may be used to contact hydrocarbon-coated surfaces in the present methods. Alternatively, cells may be removed from the cultures and the remaining medium, which has been conditioned by growth of Shewanella species cells, may be used to contact hydrocarbon-coated surfaces in the present methods. It is likely that condition medium contains biosurfactants or other biomolecules that act as wetting agents and contribute to the alterations in the wettability hydrocarbon coated surfaces.

Multiple cultures of different strains of Shewanella species may be used in the present methods. Alternatively, multiple strains may be grown in the same culture that is used in the present methods.

Treating Surface and Subsurface Formations

In the present methods, hydrocarbon-coated surfaces in surface and subsurface formations are contacted with a Shewanella species cultures in a cell containing medium or a conditioned medium. Typically the subsurface formations will be contained within an oil well site, often comprising an injection site and a production well site.

Application of the medium may include processes such as waterflooding, or the use of a fluid such as an aqueous solution or gas (such as CO₂) or a solvent or a polymer that is injected into the subsurface formation. Injection methods are common and well known in the art and any suitable method may be used. [see for example Nontechnical guide to petroleum geology, exploration, drilling, and production, 2^(nd) edition. N. J. Hyne, PennWell Corp. Tulsa, Okla., USA, Freethey, G. W., Naftz, D. L., Rowland, R. C., & Davis, J. A. (2002); and Deep aquifer remediation tools: Theory, design, and performance modeling, In: D. L. Naftz, S. J. Morrison, J. A. Davis, & C. C. Fuller (Eds.); and Handbook of groundwater remediation using permeable reactive barriers (pp. 133-161), Amsterdam: Academic Press.)].

Typically the injection site or well will communicate with the production well where oil is recovered. The application of the medium (either cell containing of cell free) may follow any number of sequences for the effective production of oil and the various options will be readily apparent to the one skilled in the art of oil recovery.

For example treatment of the subsurface formations may include pumping or adding water with Shewanella microbes via an injection well into an area comprising hydrocarbons (“treatment zone”) and allowing that water to be produced along with the recovered hydrocarbon at the production well. Treatment may also involve pumping water with cell-free medium produced by conditioning with Shewanella into a treatment zone. Treatment of an oil reservoir also may include pumping water with medium down the producer well and into the formation and then back flowing oil and water out of the producer well (huff and puff). Additionally reservoir treatment may also include inoculating an injector well that is in communication with one or more producer wells, and then subsequently providing an injection water that has been augmented with nutrients either continuously or periodically to promote growth of the Shewanella microbes, where oil is recovered at the producer well. Other treatments may include pumping water containing conditioned medium onto an environmental site comprising elements as a pile of oil sand or oil shale, collecting the water and released oil, and separating the oil from the water. The water may optionally be recycled back to be treated with Shewanella sp.

Hydrocarbon-coated surfaces may be contacted with cell containing Shewanella sp. medium or conditioned medium alone or with additional components. Additional components may be provided separately or in compositions with the medium. Components other than cultures may be injected, pumped, or otherwise applied to an area with hydrocarbon-coated surfaces prior to, together with, or following contact with cultures or conditioned medium. Mixtures of the present one or more Shewanella species and one or more electron acceptors provide compositions for use in any oil recovery or clean-up site as listed above. Electron acceptors may include, but are not limited to, nitrate, fumarate, pyruvate, ferric ion (Fe (III)) or manganese ion (Mn (IV)). Mixtures of one or more electron acceptor may be used.

Additional components of the compositions may include one or more carbon sources, such as but not limited to, lactate, yeast extract, peptone, pyruvate, glucose, succinate, formate, acetate, propionate, glutamate, glycine lysine, oil, and oil components. Oil components may be any of the many components that are present in crude oil.

The compositions may include other agents or components such as one or more additional microorganisms, such as bacteria, yeast, or fungus. Particularly useful additional microorganisms are capable of growing on oil under denitrifying conditions. In some embodiments, the additional agents may be the microorganisms Pseudomonas stutzeri strain LH4:15 (ATCC No. PTA-8823), and/or Thauera sp AL9:8, (ATCC No. PTA-9497), which are described in commonly owned and co-pending US 20090271707 A1, and US 20100078162 A1. Other agents may also include one or more chemical compounds that are not lethal to microorganisms, but are effective at degrading or partially degrading hydrocarbons and/or other contaminants.

Enhanced Oil Recovery from a Reservoir or Oil Well

Enhanced oil recovery in this context may include secondary or tertiary oil recovery of hydrocarbons from subsurface formations by techniques that alter the original properties of hydrocarbon-coated surface interface. Specifically, hydrocarbons that are adhered to surfaces within subsurface formations may be substantially liberated by contact with Shewanella sp. or biomolecules produced by these microorganisms. Typically oil is liberated on an order of about 5, 10, 15, 20, 25, 30, to about 35% of the areal coverage. These methods permit the release of oil that could not normally be recovered by waterflooding or other traditional oil recovery techniques.

Bioremediation.

In addition to applications in oil recovery the present Shewanella sp may be useful in effecting the remediation of environmental sites contaminated with hydrocarbons and other pollutants. Bioremediation strategies for hydrocarbons depend on their locations in the environment. Contamination by hydrocarbon spills can be costly to remediate and cause toxicity to environmental inhabitants. Use of microbial action as described here may provide cost-effective mechanisms for remediating hydrocarbon contamination especially under circumstances in which contamination results in hydrocarbon-coated surfaces. For example, use of Shewanella sp. and their surface active agents (such as wetting agents) help to increase wettability of soil and solubility of soil contaminants through reduction in surface and interfacial tensions. This action liberates the hydrocarbons from the surface of soils and renders them available for other remediating action, including degradation by other microbes. In this context bioremediation may be accomplished by a combination of microbes including Shewanella sp. in addition to oil-degrading microorganisms.

Shewanella Species

It has been discovered that the presence of Shewanella species or materials or biomolecules produced by Shewanella have the effect of altering the wettability of a hydrocarbon coated surface. Any and all members of the genus Shewanella have this utility.

Shewanella is a bacterial genus that has been established, in part through phylogenetic classification by rDNA and are fully described in the literature (see for example Fredrickson et al., Towards Environmental Systems Biology Of Shewanella, Nature Reviews Microbiology (2008), 6(8), 592-603; Hau et al., Ecology And Biotechnology Of The Genus Shewanella, Annual Review of Microbiology (2007), 61, 237-258).

It is within the scope of the present invention to classify relevant Shewanella on the basis of conserved regions contained in the 16S rDNA. Analysis of the 16 S rDNA from 50 different Shewanella strains revealed three conserved signature regions, 2 (SEQ ID NO:18, 19), 5, (SEQ ID NO:20,21) and 8 (SEQ ID NO: 22,23) as shown in FIG. 18, each having dominant and degenerate sequences.

To identify the Shewanella signature sequences, 50 different 16S rDNA sequences of Shewanella strains that are available in the NCBI database were aligned. The sequences are from strains that have been classified as Shewanella in the International Journal of Systematic and Evolutionary Microbiology. The sequences were aligned using the MegAlign program of the LASERGENE bioinformatics computing suite (DNASTAR Inc., Madison, Wis.). Multiple alignment of the sequences is performed using the “Clustal method of alignment” (described by Higgins and Sharp, CABIOS. 5:151-153 (1989); Higgins, D. G. et al., Comput. Appl. Biosci., 8:189-191 (1992)). For multiple alignments, the default values correspond to GAP PENALTY=10 and GAP LENGTH PENALTY=10. In addition to the Shewanella rDNA sequences, the alignment included 16S rDNA sequences of E. coli, and of microbes closely related to Shewanella, Alishewanella jeotgali, Alteromonas rubra, and Vibrio natriegenas. Through visual analysis of the 16S rDNA variable regions 2, 5, and 8, signature sequences for Shewanella species were identified and are given in FIG. 18. Thus Shewanella sp. useful in the present invention are those that comprise within the 16s rDNA the dominant or degenerate signature sequences as set forth in 2SEQ ID NO:18-23.

Specific strains of Shewanella are disclosed herein that are useful in the methods of the invention. One such strain is Shewanella putrefaciens strain LH4:18 which was isolated, identified, and deposited to the ATCC under the Budapest Treaty as #PTA-8822, as described in commonly owned and co-pending US Patent Application Publication US 2009-0260803 A1. Strain LH4:18 has the 16S rDNA sequence of SEQ ID NO:5. Examples of additional Shewanella species that may be used include but are not limited to Shewanella frigidimarina (DSM 12253), Shewanella pacifica (DSM 15445), Shewanella profunda (DSM 15900), Shewanella gelidimarina (DSM 12621), and Shewanella baltica (DSM 9439). These strains may be purchased through the German Collection of Microorganisms and Cell Cultures (DSMZ). These and other strains that may be used have at least about 94%, 95%, 96%, 97%, 98%, or 99% identity to SEQ ID NO:5 of strain LH4:18.

Additionally useful strains are Shewanella strains EH60:12, EH60:2, and EH60:10, which were identified herein and characterized with partial 16S rDNA sequences of SEQ ID NOs:15, 16, and 17, respectively. Shewanella species include microorganisms having a 16S rDNA sequence with at least about 95%, 96%, 97%, 98%, or 99% identity to any one or all of SEQ ID NOs:15-17.

In addition to the known Shewanella sp. described above, the invention provides a newly identified Shewanella sp. which is useful in the present methods. This new strain is identified as Shewanella sp. strain L3:3 which has been deposited with the ATCC under the Budapest Treaty as strain PTA-10980 Shewanella sp. strain L3:3 was isolated from an injection water sample obtained from the Alaskan North Slope and has the 16S rDNA sequence of SEQ ID NO:3. Within the 16S rDNA sequence are signature sequences that were identified in variable regions 3 and 6 of prokaryote rDNA that have nucleotide sequences of SEQ ID NOs: 13 and 14, respectively. As shown in FIG. 14, the nucleotides at specific positions (with respect to the first nucleotide of SEQ ID NO:3) 438-40, 451, 454-57, 466-69, 471, 484-86 and 496 within SEQ ID NO:13 are different in strain L3:3 from the nucleotides present in the 16S rDNA of Shewanella putrefaciens, Shewanella sp. LH4:18 and Shewanella algae. As shown in FIG. 15, the nucleotides at specific positions (with respect to the first nucleotide of SEQ ID NO:3) 995-6, 1001-05, 1007, 1012, 1014, 1016-1018 and 1035 within SEQ ID NO:14 are also different in strain L3:3 from the nucleotides present in the 16S rDNA of Shewanella putrefaciens, Shewanella sp. LH4:18 and Shewanella algae. Shewanella strains found herein to have the same nucleotides at all of these positions are Shewanella sp. C31, Shewanella sp. L-10, Shewanella chilikensis JC5T, Shewanella sp. C16-M, and a Shewanella clone identified as D00402024H07. While having the signature sequences of SEQ ID NOs:13 and 14, the present Shewanella species that are closely related to the newly identified strain L3:3 have at least about 97%, 98% or 99% sequence identity to the DNA sequences for 16S ribosomal RNA of SEQ ID NO:3. In addition, strains closely related to strain L3:3 have a riboprint pattern identifier of 212-824-S-4 as demonstrated in FIG. 16. This riboprint pattern was identified herein for Shewanella sp. strain L3:3.

Shewanella sp. are gram negative, metal-reducing bacteria that are capable of reducing a wide range of terminal electron acceptors. These microorganisms gain energy to support anaerobic growth by coupling the oxidation of H₂ or organic matter to the redox transformation of a variety of multivalent metals, which leads to the precipitation, transformation, or dissolution of minerals.

On the basis of the 16S rDNA sequences isolated from the above described Shewanella sp. and using the alignment methods described herein, it has been discovered that all bacteria having a 16S rDNA sequence that is at least 89% identical to either the full length 16S rDNA as set forth in either SEQ IC NO:3 (L3:3) or 5(LH4:18) must be classified as Shewanella.

EXAMPLES

The present invention is further defined in the following Examples. It should be understood that these Examples, while indicating preferred embodiments of the invention, are given by way of illustration only. From the above discussion and these Examples, one skilled in the art may ascertain the essential characteristics of this invention, and without departing from the spirit and scope thereof, may make various changes and modifications of the invention to adapt it to various usages and conditions.

Additional Abbreviations Used in the Examples

The meaning of abbreviations is as follows: “hr” means hour(s); “mL” means milliliter; “° C.” means degrees Celsius; “mg” means milligram(s); “mm” means millimeter; “g” means gram(s); “GC” means gas chromatography; “g of oil/g of total fluid” means gram of oil per gram of total fluid; “ppm” means part per million; “mM” means millimolar; “%” means percent; “CFU/mL” means colony forming unit per milliliter; “LB” means Luria broth medium; “min” means minute(s); “mL/min means milliliter per minute; “NIC” means non-inoculated control (negative controls in microbial culture experiments); “μg/L” means microgram per liter; “nM” means nanomolar; “μM” means micromolar.

General Methods

Growth of Microorganisms

Techniques for growth and maintenance of anaerobic cultures are described in “Isolation of Biotechnological Organisms from Nature”, (Labeda, D. P. ed. 117-140, McGraw-Hill Publishers, 1990). When using nitrate as an electron acceptor in anaerobic cultures, growth is measured by nitrate depletion from the growth medium over time. Nitrate is utilized as one of the primary electron acceptors under the growth conditions used herein. The reduction of nitrate to nitrogen has been previously described (Moreno-Vivian, C., et al., J. Bacteriol., 181, 6573-6584, 1999). In some cases nitrate reduction processes lead to nitrite accumulation, which is subsequently further reduced to nitrogen. Accumulation of nitrite is therefore also considered evidence for active growth and metabolism by microorganisms.

Ion Chromatography

An ICS2000 chromatography unit (Dionex, Banockburn, Ill.) was used to quantitate nitrate and nitrite ions in growth medium. Ion exchange was accomplished on an AS15 anion exchange column using a gradient of 2 to 50 mM potassium hydroxide. Standard curves were generated and used for calibrating nitrate and nitrite concentrations.

Genomic DNA Extractions from Bacterial Cultures

To extract genomic DNA from liquid bacterial cultures, cells were harvested by centrifugation (10,000 rpm, at room temperature) and resuspended in lysis buffer (100 mM Tris-HCL, 50 mM NaCl, 50 mM EDTA, pH8.0) followed by agitation using a Vortex mixer. Reagents were then added to a final concentration of 2.0 mg/mL lysozyme, 10 mg/mL SDS, and 10 mg/mL Sarkosyl to lyse the cells. After further mixing with a Vortex mixer, 0.1 mg/mL RNase and 0.1 mg/mL Proteinase K were added to remove RNA and protein contaminants, and the samples were incubated at 37° C. for 1.0-2.0 hr. Post incubation, the samples were extracted twice with an equal volume of a phenol:chloroform:isoamyl alcohol (25:24:1, v/v/v) and once with chloroform: isoamyl alcohol (24:1). One-tenth volume of 5.0 M NaCl and two volumes of 100% ethanol were added to the aqueous layer, and mixed. The tubes were frozen at −20° C. overnight and then centrifuged at 15,000×g for 30 min at room temperature to pellet chromosomal DNA. The pellets were washed once with 70% ethanol, centrifuged at 15,000×g for 10 min, dried, resuspended in 100 μL of de-ionized water and stored at −20° C. An aliquot of the extracted DNA was visualized on an agarose gel to ascertain the quantity and quality of the extracted DNA.

Direct Colony rDNA Sequence Analysis

Genomic DNA from bacterial colonies was isolated by diluting bacterial colonies in 50 μL of water or Tris-HCL buffer pH7-8. Diluted colony DNAs were amplified with Phi 29 DNA polymerase prior to sequencing (GenomiPHI Amplification Kit GE Life Sciences, New Brunswick, N.J.). An aliquot (1.0 μL) of a diluted colony was added to 9.0 μL of the Lysis Reagent (from the GenomiPHI Amplification Kit) and heated to 95° C. for 3 min followed by immediate cooling to 4° C. 9.0 μL of Enzyme Buffer and 1.0 μL of Phi 29 enzyme were added to each lysed sample followed by incubation at 30° C. for 18 hr. The polymerase was inactivated by heating to 65° C. for 10 min followed by cooling to 4° C.

DNA sequencing reactions were set up as follows: 8.0 μL of GenomiPHI amplified sample were added to 8.0 μL of BigDye v3.1 Sequencing reagent (Applied Biosystems, Foster City, Calif.) followed by 3.0 μL of 10 μM primers SEQ ID NO: 1 in combination with SEQ ID NO: 2 (prepared by Sigma Genosys, Woodlands, Tex.), 4.0 μL of 5× BigDye Dilution buffer (Applied Biosystems) and 17 μL Molecular Biology Grade water (Mediatech, Inc., Herndon, Va.). Sequencing reactions were heated for 3 min at 96° C. followed by 200 thermocycles of (95° C. for 30 sec; 55° C. for 20 sec; 60° C. for 2 min) and stored at 4° C. Unincorporated fluorescently labeled ddNTPs were removed using Edge Biosystems (Gaithersburg, Md.) clean-up plates. Amplified reactions were pipetted into wells of a pre-spun 96 well clean up plate. The plate was centrifuged for 5 min at 5,000×g in a Sorvall RT-7 (Sorvall, Newtown, Conn.) at 25° C. The cleaned up reactions were placed directly onto an Applied Biosystems 3730 DNA sequencer and sequenced with automatic base-calling.

Each of the assembled rDNA sequences was compared to the NCBI rDNA database (˜260,000 rDNA sequences) using the BLAST algorithm (Altschul et al., supra). The primary hit was used as an identifier of the most closely related known species identification. The initial screen using the rDNA colony direct sequencing reduced the number of colonies to be carried through further screening by 20 fold. Automated Ribotyping

Automated ribotyping was used for identification of selected strains with similar 16S rDNA sequence phylogenetic characteristics (Webster, John A, 1988. U.S. Pat. No. 4,717,653; Bruce, J. L., Food Techno., (1996), 50: 77-81; and Sethi, M. R., Am. Lab. (1997), 5: 31-35). Ribotyping was performed as recommended by the manufacturer (DuPont Qualicon Inc., Wilmington, Del.). For these analyses, one fresh colony was picked, resuspended in the sample buffer and added to the processing module for the heat treatment step at 80° C. for 10 min to inhibit endogenous DNA-degrading enzymes. The temperature was then reduced and lytic enzymes lysostaphin and N-acetyl-muramidase, provided by the manufacturer, were added to the sample. The sample carrier was then loaded onto the Riboprinter system with other commercial reagents. Restriction enzyme digestion using EcoRI enzyme, gel electrophoresis and blotting steps were completely automated. Briefly, bacterial DNA was digested with the EcoRI restriction enzyme and loaded onto an agarose gel, restriction fragments were separated by electrophoresis and then transferred to a nylon membrane. After a denaturation step, the nucleic acids were hybridized with a sulfonated DNA probe containing the genes for the small and large rRNA subunits of E. coli, the 5S, 16S, and 23S ribosomal rRNAs. The hybridized labeled-probe was detected by capturing light emission from a chemiluminescent substrate with a charge-coupled device camera. The output consisted of a densitometry finger scan depicting the specific distribution of the EcoRI restriction fragments containing the genomic rDNA sequences and their molecular weights, which are particular to the genomic DNA sequence of a specific strain independent of the 16S rDNA sequence.

Measuring the Potential for the Microbes to Release Oil from Sand Particles

In order to screen test cultures for the ability to release oil from the nonporous silica medium, a microtiter plate assay to measure the ability of the microbes to release oil/sand from oil-saturated North Slope sand was developed. The assay is referred to as the LOOS test (Less Oil On Sand). Briefly, autoclaved North Slope sand was dried under vacuum at 160° C. for 48 hr. Twenty grams of the dried sand was then mixed with 5 mL of autoclaved, degassed crude oil. The oil-coated sand was then allowed to age anaerobically at room temperature, in an anaerobic chamber, for at least a week. Microtiter plate assays were set up and analyzed in an anaerobic chamber. Specifically, 2 mL of test cultures were added into the wells of a 12-well microtiter plate (Falcon Multiwell 12 well plates, #353225, Becton Dickinson, Franklin Lakes, N.J.). The control wells contained 2 mL of the medium alone. Approximately 40 mg of oil-coated sand was then added to the center of each well. Samples were then monitored over time for release and accumulation of “free” sand that collected in the bottom of the wells. Approximate diameters (in millimeters) of the accumulated total sand released were measured. A score of 2 mm and above indicates the microbes' potential to release oil from the nonporous silica medium.

Gas Chromatography for Determining Residual Oil on Sand

A gas chromatography (GC) method was developed to analyze the sand from sandpacks for residual oil. An empirical relationship was determined based on the North Slope sand and the intrinsic pore volume of packed sand, e.g., for 240 g of packed sand there is a pore volume of 64 mL. Weights of the individual sand samples were obtained and the oil on the sand was extracted with a known amount of toluene. A sample of this toluene with extracted oil was then analyzed by GC. A calibration curve was generated and used to determine the amount of oil in toluene on a weight percent basis. This was then multiplied by the total amount of toluene used to extract the oil resulting in the total amount of oil on the sand. This value was then divided by the total sample weight to yield the percent of oil with respect to the total sample weight. The weight percent of oil of the sample was multiplied by the ratio of the empirically derived characteristic of packed North Slope sand (total weight of sample after being flooded with brine divided by total sand weight, 1.27). This relationship was equal to the amount of oil on dry sand. This value was then multiplied by the ratio of the weight of North Slope sand to the weight of fluid trapped in the pore space of the sand, 3.75. This resulting value was the residual oil left on the sand in units of g of oil/g of total fluid in the pore space.

Growth Medium and Growth Protocol

PPGAS medium was used in the following Examples unless stated otherwise. The medium contained: 1.6 mM MgSO₄, 20 mM KCl, 20 mM NH₄Cl, 120 mM Tris base 0.5% glucose and 1% Bacto peptone. The initial culture was grown aerobically in the medium at 25° C.

Sterile injection brine (SIB) contained: 198 mM NaCl, 1 mM MgCl₂, 1.8 mM CaCl₂, 1.2 mM KCl, 16 mM NaHCO₃, 0.05 mM SrCl₂, 0.13 mM BaCl₂, 0.14 mM LiCl) plus 1% peptone.

2 below:

TABLE 2 Composition of the SL10 Medium Final Chemical Growth component Concentration Source Nitrogen 18.7 mM NH₄Cl Phosphorus 3.7 mM KH₂PO₄ Magnesium 984 μM MgCl₂•6H₂O Calcium 680 μM CaCL₂•2H₂O Sodium chloride 172 mM NaCl Trace metals 7.5 μM FeCl₂•4H₂O 12 nM CuCl₂•2H₂O 500 nM MnCL₂•4H₂O 800 nM CoCl₂•6H₂O 500 nM ZnCl₂ 97 nM H₃BO₃ 149 nM Na₂MoO₄•2H₂O 100 nM NiCl₂•6H₂O Selenium-tungstate 22.8 nM Na₂SeO₃•5H₂O 24.3 nM Na₂WO₄•2H₂O pH buffer/Bicarbonate 29.7 mM NaHCO₃ Vitamins 100 μg/L vitamin B12 80 μg/L p-aminobenzoic acid 20 μg/L D(+)-Biotin 200 μg/L nicotinic acid 100 μg/L calcium pantothenate 300 μg/L pyridoxine hydrochloride 200 μg/L thiamine-HCL•2H₂O 50 μg/L Alpha-lipoic acid The pH of the medium was adjusted to between 7.4-7.8.

Example 1 Comparison of the Ability of Early and Late Stage Microbial Cultures to Release Oil from Sand Particles

To determine whether late stationary phase growth enhances oil release, the oil release activity of an anaerobic overnight culture of strain LH4:18 was compared to that of a one week old culture of the same strain. A culture was grown initially as described above in PPGAS medium. It was then moved into an anaerobic chamber, was supplemented with 500 ppm sodium lactate and 1000 ppm sodium nitrate, and divided in half. One half was used immediately in an anaerobic LOOS test, described in General Methods. The other half (Week1 culture) was aged (left for a week in the anaerobic chamber) and then the LOOS test was performed using this culture.

FIG. 1 shows the relative sand release by strain LH4:18 cultures over a period of three weeks. After about 6 days, a 6 mm zone of released sand was observed in the bottom of the wells for the week old (week 1) culture and a 3 mm zone was observed for the day-old sample (Day 1). Thus these results indicate that late stationary phase growth cultures may be more effective in expression of wetting agent molecules in that the rate of the sand/oil release was higher for the week old sample and continued to increase with time.

Example 2 Demonstration of Oil Release During Both Aerobic and Anaerobic Growth

To ascertain whether oil release occurs when the assay is performed aerobically versus anaerobically, and whether the addition of lactate and nitrate are beneficial, the following experiment was performed. A LOOS test was set up as described above. A culture of strain LH4:18 was grown aerobically overnight at 25° C. in the PPGAS medium. It was then divided in half. One half was supplemented with 1000 ppm sodium lactate and 2000 ppm sodium nitrate. The other half received no further supplements. Each of these cultures was then divided into an aerobic set and an anaerobic set. LOOS tests were set up to compare the samples. PPGAS medium alone samples, with and without the respective supplements, were used as controls.

The results showed that the sand/oil release was relatively the same irrespective of whether the assay was performed aerobically or anaerobically (FIG. 2). Interestingly, the addition of lactate and nitrate had a detrimental effect on both aerobic and anaerobic cultures. It should be noted, however, that even with the aerobic cultures, oxygen could still be limiting due to the high cell density.

Example 3 Comparison of Electron Acceptors and their Effect on Oil Release by Strain LH4:18

A survey of the literature shows that fumarate may act as an efficient terminal electron acceptor (Morris, C. J., et al., Biochem. J., 302: 587-593, 1994). In addition, in Shewanella species, certain cell surface and respiratory molecules are more abundant in cells grown with fumarate, rather than nitrate or iron citrate, as the terminal electron acceptor (Morris et al., supra). In Example 2, it was demonstrated that nitrate addition was detrimental in oil/sand release. Fumarate was therefore tested as an acceptable and possibly more advantageous replacement in this assay.

A frozen stock culture of strain LH4:18 was diluted 1:100 in SIB plus 1% peptone and placed into an anaerobic chamber. The culture was then split and sodium nitrate (2000 ppm), both sodium lactate (1000 ppm) and sodium nitrate (2000 ppm), sodium fumarate (2000 ppm), or both sodium lactate and sodium fumarate supplements were added to different samples. The control sample contained no additional supplements. Samples were grown anaerobically for 3 days. On the second day, samples were fed again with their respective supplements. MPNs were monitored at Day 1 and again after 3 days of anaerobic growth. On Day 3, a LOOS test was set up and sand/oil release was compared across all samples over time.

FIG. 3 shows a comparison of CFU/mL, expressed as Log 10 (MPN), on the day of the LOOS test set up (Day 3) and the relative sand release for each sample. The results show that even though growth was relatively the same across all conditions, the sand/oil release was better for samples containing fumarate instead of nitrate as the terminal electron acceptor.

Example 4 Demonstration of the Effect of Various Media Formulations on Oil Release by Strain LH4:18

For certain bacterial species, glucose is necessary for the expression of some surface molecules and surfactants. To determine whether glucose can improve oil release using strain LH4:18, a LOOS test with this strain grown aerobically overnight in PPGAS medium with and without glucose was performed. The samples were then placed into an anaerobic chamber and the LOOS test was performed anaerobically as described above.

FIG. 4 shows that the sand/oil release response was relatively the same whether glucose was present or not.

In order to determine if the effect of strain LH4:18 on oil release was limited to a rich medium, the LOOS test response was measured using different media. Media tested were PPGAS, LB, and supplemented simulated injection brine (SIB). SIB was supplemented with 1% peptone and either MgSO₄ and KCl, NH₄CL, or Tris. Cultures of strain LH4:18 were grown aerobically overnight. Samples were then placed into an anaerobic chamber and the LOOS test was performed anaerobically.

The simulated injection brine with 1% peptone added worked as well as the other rich medium formulations as shown in FIG. 5. Strain LH4:18 grew relatively the same in each of the media. All cultures exhibited about the same sand/oil release response in the LOOS test.

To determine whether yeast extract worked as well as peptone in the simulated injection brine, these supplements were compared directly in a LOOS assay. Strain LH4:18 was grown aerobically overnight at 25° C. in SIB supplemented with 1% peptone or 1% yeast extract (YE). After 20 hr, the SIB/peptone culture had approximately 4.27E+09 CFU/mL and the SIB/YE culture contained about 9.33E+09 CFU/mL. The samples were then placed into the anaerobic chamber and the LOOS test was performed anaerobically.

The data in FIG. 6 shows that YE may be substituted for peptone with no detrimental effect on the oil release response.

Example 5 Demonstration of Oil Release by Culture Supernatant

A number of microbial species release surfactants in their surrounding media. To determine whether a wetting agent from strain LH4:18 might be released into the surrounding medium, a LOOS test was performed using both a whole LH4:18 culture and also the supernatant alone of an LH4:18 culture. Strain LH4:18 was grown aerobically overnight at 25° C. in SIB supplemented with 1% peptone. After 20 hr, the culture contained approximately 1.49E+09 CFU/mL. The culture was then divided into two aliquots and one aliquot was centrifuged at 12000×g for 3 min to remove the cells. The supernatant was collected from the centrifuged sample and transferred into a new tube. Both samples were then placed into an anaeriobic chamber and the LOOS test was performed anaerobically as described above.

FIG. 7 shows that the supernatant alone released the sand/oil as effectively as the whole culture indicating that an agent affecting oil release was present in the medium.

While the Example above showed that the supernatant alone released the sand/oil almost as effectively as the whole culture, an experiment was performed to determine if oil release ability remained surface bound. A culture of strain LH4:18 was grown overnight at 25° C. in SIB supplemented with 1% peptone. The culture was then divided into two aliquots and half was centrifuged at 12000×g for 3 min to remove the cells. The supernatant was collected from the centrifuged sample and transferred into a new tube. The pellet was then resuspended in fresh medium. The other half of the overnight culture was also centrifuged and the supernatant was filtered (Supor, 0.2 μm, Pall Corp., Ann Arbor, Mich.) to remove the microorganisms. The three samples (centrifuged supernatant, filtered supernatant, and resuspended cells) were then placed into the anaerobic chamber and the LOOS test was performed anaerobically. FIG. 8 shows that both supernatant samples released the oil/sand equally well, while oil release by the resuspended cells was less effective. However the resuspended cells were able to cause some oil release.

Example 6 Effect of Strain LH4:18 in Combination with Pseudomonas stutzeri Strain LH4:15 in Oil Release

To determine whether the oil release effected by strain LH4:18 is compromised by the presence of other microbes, a LOOS test was performed on strain LH4:18 alone and also in the presence of Pseudomonas stutzeri LH4:15 (ATCC No. PTA-8823). Specifically, cultures of strains LH4:15 and LH4:18 were grown separately overnight in the PPGAS medium. Three LOOS tests were performed: 1) using strain LH4:15 alone; 2) using strain LH4:18 alone; and 3) using the combined cultures. The results shown in FIG. 9 indicate that the oil release ability of strain LH4:18 was not adversely affected by the presence of the other microorganism.

Example 7 Measuring the Effects of Other Shewanella Species in Oil Release

Additional Shewanella strains had been identified through anaerobic enrichments on oil production fluids, using SL10 medium and Fe(III) as the electron acceptor. Strains EH60:12, EH60:10, and EH60:2 were identified as Shewanella species by their 16S rDNA sequences (SEQ ID NOs:15, 16, and 17, respectively). These strains were grown aerobically overnight in the LB medium. A LOOS test was set up on 2 mL of the whole cultures as previously described.

The results in FIG. 10 demonstrate that other Shewanella species (e.g., strains EH60:12, EH60:2, and EH60:10) were also capable of releasing oil. Results were comparable to those of strain LH4:18.

Other known Shewanella species were purchased through the German Collection of Microorganisms and Cell Cultures (DSMZ): Shewanella frigidimarina (DSM 12253), S. pacifica (DSM 15445), S. profunda (DSM 15900), S. gelidimarina (DSM 12621), and S. baltica (DSM 9439). Cultures of each strain were grown aerobically overnight in SIB supplemented with 1% peptone. The cultures were then split and 1000 ppm sodium lactate and 2000 ppm sodium nitrate, or 1000 ppm sodium lactate and 3715 ppm sodium fumarate were added. A LOOS test was performed on 2 mL of the cultures as previously described. Samples were not adjusted for growth.

FIG. 11 shows that these known Shewanella species also released oil in the LOOS assay. As in Example 3, those samples grown in the presence of fumarate as the electron acceptor performed better than those grown in the presence of nitrate.

Example 8 Shewanella Increases the Contact Angle of Oil in Deep Sediment Sand

Strain LH4:18 was grown aerobically in PPGAS medium and added to a LOOS test as described above. After approximately two weeks, an aliquot of the sand was removed from the bottom of the strain LH4:18 well and was compared microscopically to oil coated sand from a medium alone control well. FIG. 12 shows photomicrographs for comparison. FIG. 12A shows the untreated oil coated sand. As indicated by the lines drawn on the picture, the contact angle between the hydrocarbon and sand is low indicating that the surface energy encourages the hydrocarbon to coat the entire mineral grain. The right photomicrograph in FIG. 12B shows the effect of exposure to strain LH4:18. As indicated by the lines drawn on the picture, the contact angle has increased dramatically indicating a significant change in the surface energy between the hydrocarbon and the mineral, and showing substantial liberation of hydrocarbon from the surface of the sand particle. This is a visual demonstration of change in wettability.

Example 9 Measuring Oil Release from Sandpacks

Oil Release Sandpack or Core Flood Assay

The potential application of strain LH4:18 in MEOR treatment was evaluated using the sandpack technique. This was done with an in-house developed Teflon® shrink-wrapped sandpack apparatus. Using a 0.5 inches (1.27 cm) OD and 7 inches (17.78 cm) long Teflon heat shrink tube, an aluminum inlet fitting with Viton® O-ring was attached to one end of the tube by heat with a heat gun. North Slope sand was added to the column which was vibrated with an engraver to pack down the sand and release trapped air. A second aluminum inlet fitting with Viton® O-ring was attached to the other end of the tube and sealed with a heat gun. The sandpack was then put in an oven at 275° C. for 7 min to evenly heat and shrink the wrap. The sandpack was removed and allowed to cool to room temperature. A second Teflon® heat shrink tube was installed over the original pack and heated in the oven as described above. After the column had cooled, a hose clamp was attached on the pack on the outer wrap over the O-ring and then tightened.

Four sandpack columns were flooded horizontally with three pore volumes of SIB1 low bicarbonate (same as SIB but with 1 mM bicarbonate) at 10 mL/min via a syringe pump and a 60 mL (Becton Dickinson, Franklin Lakes, N.J.) sterile plastic polypropylene syringe. All four sandpacks were then flooded with two pore volumes of anaerobic autoclaved crude oil at 0.5 mL/min to achieve irreducible water saturation. The crude oil was aged on the sand for three weeks before inoculating. For the inoculation culture, strain LH4:18 was grown aerobically overnight in PPGAS medium. The culture was then placed in an anaerobic environment where Na-Lactate was added to 1000 ppm and Na-Nitrate was added to 2000 ppm. This sample was anaerobically aged for 5 days before inoculating the sandpacks. Two columns were anaerobically inoculated with a sample of strain LH4:18 for one pore volume at 0.4 mL/hr. Two control sandpacks were flooded using anaerobic SIB1 low bicarbonate using the same inoculation procedure. The four sandpacks were then shut-in for incubation with the oil for five days. After the shut-in, the columns were produced by flushing with anaerobic sterile SIB low bicarbonate at 0.4 mL/hr for three pore volumes to prepare the production flood.

At the conclusion of the production flood, the 7 inches (17.78 cm) slim tubes were sacrificed into 5 one-inch sections labeled A-E. One inch was skipped at the beginning and at the exit of the slim tube to avoid edge effects during analysis. Sections A, C, and E were analyzed for residual oil saturation on the sand by the GC method described in General Methods.

The results in FIG. 13 show that average residual oil saturation in the uninoculated column was 22.5% whereas the residual oil saturation for strain LH4:18 inoculated columns was 16.1%, indicating that strain LH4:18 was able to reduce residual oil saturation by approximately 6.5%.

Example 10 Discovery of Oil Recovery Activity in Live Injection Water Sample

To screen enrichment cultures, environmental samples or isolated strains for the ability to release oil from a nonporous silica medium, a microtiter plate assay was developed to measure the ability of microbes to release oil/sand from oil-saturated North Slope sand. North Slope sand was autoclaved and then dried under vacuum at 160° C. for 48 hr and 20 g of this dried sand was then mixed with 5 mL of autoclaved, degassed crude oil obtained from Milne point, North Slope. The oil-coated sand was then allowed to adsorb to the sand and age anaerobically at room temperature for at least a week. Microtiter plate assays were set up in a Coy anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.). The assay is referred to as the LOOS test (Liberation of Oil Off Sand).

Water samples were obtained from production and injection well heads as mixed oil/water liquids in glass 1.0 L brown bottles, filled to the top, capped and sealed with tape to prevent gas leakage. Gas from inherent anaerobic processes sufficed to maintain anaerobic conditions during shipment. The bottles were shipped in large plastic coolers filled with ice blocks to the testing facilities within 48 hr of sampling.

A sample of non sterile (‘Live’) injection water obtained from Alaskan North Slope was used in a LOOS test plus and minus Shewanella putrefaciens strain LH4:18 (ATCC No. PTA-8822) to determine the efficacy of the Shewanella LH4:18 surface active agent in a background microbial population simulated by the live injection water. Live water was included in the LOOS test as a control. A positive LOOS result was obtained for live injection +/−LH4:18 microbial treatments. The oil/sand release scores obtained from these LOOS tests are given in Table 3.

TABLE 3 Response of Live Injection Water vs. Shewanella LH4:18 in the Release of Oil from Sand in the LOOS Test Time in days Live 0 3 7 10 18 26 Test Injection Response as diameter of Sample Water LH4: 18 Nutrients¹ sand released (mm) L1 + − none 0 1 2 4 4 4 L2 + − N 0 1 2 3 3 3 L3 + − L/N 0 5 6 6 7 7 L4 + − F 0 2 2 4 5 5 L5 + − L/N 0 2 3 4 6 6 L6 + + none 0 4 4 4 5 5 L7 + + N 0 2 4 4 4 4 L8 + + L/N 0 4 5 6 6 6 L9 + + F 0 4 5 5 6 6  L10 + + L/N 0 3 5 6 6 6 ¹N = Nitrate (2000 ppm); L/N = Lactate (1000 ppm) plus Nitrate (2000 ppm); F = Fumarate (2000 ppm)

The degree of oil release response is measured as the diameter of the sand released from oil. The data demonstrates that test sample L3 consisting of live injection water released oil faster than the other samples. This sample was not inoculated with Shewanella LH4:18. This test demonstrates that the live injection water contained an agent or agents that facilitated the release of oil from sand independent of Shewanella sp LH4:18.

Example 11 Isolation and Identification of Shewanella Species in Oil Reservoir Production Water

Aliquots of the live injection water giving positive oil release results in the LOOS test were streaked on LB agar plates (Teknova, Hollister, Calif.) in order to isolate and identify those strain(s) present in live injection water capable of oil release. Representative colonies with unique morphologies were isolated from the live injection water test samples. Samples of these isolated colonies were screened by PCR amplification using direct colony rDNA analysis described in the General Methods using both the reverse PCR primer 1492r (SEQ ID NO:1) and forward PCR primer 8f (SEQ ID NO:2). The resultant rDNA sequence from each colony was aligned and matched with the GenBank sequence database for phylogenetic strain identification.

One isolate, named L3:3, was identified as having 16S rDNA homology to Shewanella sp C16-M. Both L3:3 and C16-M strains as well as four other reported Shewanella isolates (C31, L31, C13-M and JC5T) have 16S rDNA sequences that are similar to a newly proposed Shewanella species, Sh. chilikensis (K. Sucharita et al, (2009) International Journal of Systematic and Evolutionary Microbiology 59:3111-3115). The 16S rDNA sequence of L3:3 has 99.9% identity to three of the six rDNA gene sequences in the GenBank database that could be classified as Shewanella chilikensis: strain JC5T, strain C16-M, and sequence from a population study designated Shewanella clone D004024H07. Shewanella chilikensis JC5T was isolated from a lake mud environment, Shewanella chilikensis C16-M was isolated from a marine environment and Shewanella clone D004024H07 was isolated (by DuPont) from environmental samples taken from an Alaskan oil well (Pham, V. D, et al., Environ. Microbiol. 11:176-187 2009).

Strain L3:3 was identified to be Shewanella sp L3:3 and was further characterized by DNA sequence analysis to have signature sequences within Shewanella species rDNA sequences. Specifically, Shewanella sp L3:3 was found to have 16S rDNA sequence (SEQ ID NO: 3) and signature sequences within Shewanella 16S rRNA variable regions 3 and 6 that are defined in SEQ ID NO:13 (within the prokaryote 16S rRNA variable region 3) and SEQ ID NO: 14 (within the prokaryote 16S rRNA variable region 6). These signature sequence regions were discovered when the 16S rDNA sequence profile of Shewanella sp L3:3 was aligned with 42 published 16S rDNA sequences of Shewanella sp., which were pared down to the nine sequences (SEQ ID NO:4 through 12) in FIGS. 1 and 2 for demonstration of the variations. Shewanella sp L3:3 full 16S rDNA sequence (SEQ ID NO: 3) was used as the alignment anchor. FIG. 14 shows signature base variations that occur in L3:3 in the 16S rRNA variable region 3 and SEQ ID NO: 13 (bp coordinates 430 to 500) at specific coordinate positions: 438-40, 451, 454-57, 466-69, 471, 484-86 and 496 and are observed as signature in nature when compared across 16S rDNA of various Shewanella species. A similar observation was made for bacterial variable region 6 for sequences closely related to Shewanella sp L3:3, e.g., sequences similar to that defined by FIG. 15 and SEQ ID NO: 14 can be found in published sequences. Strain variations occur between base coordinates 990 and 1049, specifically at positions: 995-6, 1001-5, 1007, 1012, 1014, 1016-18 and 1035.

In addition to strain L3:3, there are six Shewanella 16S rDNA-like sequences, which were found in sequence databases, that contain the diagnostic signature sequences within variable regions 3 and 6 that are similar to those defined by SEQ ID NO: 13 and SEQ ID NO: 14. This Shewanella group includes: uncultured bacterium clone D004024H07 (NCBI GenBank accession No. gb|EU721813|), Shewanella sp C16-M (gb|EU563338.1|), Shewanella sp. L-10 (gb|DQ164801.1|), Shewanella sp. C31 (gb|EU563345.1|) and Shewanella Sp. JC5T (sp.=chilikensis) (gb|FM210033.2|). Shewanella sp. C13-M (gb|EU563337.1|) does not have the position 471 nucleotide of the L3:3 diagnostic signature.

All strains were isolated from marine environment, oil fields or the bottom of a lagoon. None of these strains at the time of this invention were available from the ATCC or DSMZ public depositories to allow for ribotyping comparisons.

Example 12 Riboprint Analysis of Strain L3:3

To further characterize Shewanella strain L3:3, preparations of this strain were analyzed by Riboprinter® and compared to 7525 patterns contained within DuPont Environmental Services and Qualicon libraries compiled from samples taken all over DuPont as well as another 6950 patterns that DuPont Qualicon has supplied from standard identified organisms. Based on the analyses of Riboprint batch 052009 (FIG. 16), which provides a chromosomal fingerprint of the tested strains, it is clear that the riboprint pattern for strain L3:3 (sample 1) constitutes a riboprint which is unique when compared against the available DuPont Riboprint Libraries and is designated as ribogroup identifier 212-824-S-4. It is probable for various strains to share single similar riboprint bands generated by hybridizing the labeled E. coli rDNA operon probe to each strain's genomic Eco RI fragments, but it is the overall riboprint banding pattern that constitutes identification of a given strain in a specific riboprint or ribogroup identifier.

Example 13 Enhanced Oil Release by Strain L3:3

The purified strain L3:3 was tested in a LOOS test designed to identify the strains' efficacy in altering the surface tension of oil coated silica particles. Strain L3:3 clearly contributed to oil release from sand as compared to the efficiency of oil release by Shewanella strain LH4:18 (ATCC No. PTA-8822) as shown in Table 4. Both strains exhibited release of oil/sand from oil coated particles. The ability to release oil/sand was similar when fumarate was the electron acceptor for both Shewanella strains tested (LH4:18 and L3:3), but L3:3 appeared to have greater release as compared to LH4:18 when nitrate was used as the electron acceptor.

TABLE 4 LOOS test: Oil/sand Release Response for Purified Cultures of Shewanella strains L3:3 and LH4:18 Time in Days 0 2 5 7 9 12 14 Electron Response as diameter of sand Test Strain receptor released (mm) 1 L3:3 none 0 4 6 7 7 8 8 2 L3:3 L/N¹ 0 2 5 5 7 7 8 3 L3:3 L/F² 0 3 7 7 7 8 8 4 LH4:18 none 0 2 6 7 7 7 7 5 LH4:18 L/N 0 0 3 3 3 4 4 L6 LH4:18 L/F 0 3 6 7 7 7 7 ¹lactate plus nitrate ²lactate plus fumarate

Example 14 Prophetic Anaerobic Growth of Strain L3:3 on Oil as the Sole Carbon Source

To study growth of strain L3:3 as compared to Shewanella LH4:18, purified isolates are inoculated into 20 mL serum vials containing ˜10 mL minimal salts medium (Table 5), 1.6 g/l sodium nitrate and 5.0 mL of autoclaved crude oil. The medium is deoxygenated by sparging the filled vials with a mixture of nitrogen and carbon dioxide followed by autoclaving. All manipulations of bacteria are done in an anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.). The cultures are incubated at ambient temperatures with moderate shaking (100 rpm) for several weeks to several months and monitored for nitrate, nitrite, visible turbidity and visible oil modifications. When the nitrate is depleted in any culture, sodium nitrate at 50 g/l is added to bring its concentration in the medium up to 0.4 g/l sodium nitrate.

TABLE 5 Minimal salts medium Final Chemical Growth component concentration Source Nitrogen 18.7 μM NH₄Cl Phosphorus 3.7 μM KH₂PO₄ Magnesium 984 μM MgCl₂•6H₂O Calcium 680 μM CaCL₂•2H₂O Sodium chloride 172 mM NaCl Trace metals 670 μM nitrilotriacetic acid 15.1 μM FeCl₂•4H₂O 1.2 μM CuCl₂•2H₂O 5.1 μM MnCL₂•4H₂O 12.6 μM CoCl₂•6H₂O 7.3 μM ZnCl₂ 1.6 μM H₃BO₃ 0.4 μM Na₂MoO₄•2H₂O 7.6 μM NiCl₂•6H₂O pH buffer (7.5 final) 10 mM Hepes Selenium-tungstate 22.8 nM Na₂SeO₃•5H₂O 24.3 nM Na₂WO₄•2H₂O Bicarbonate 23.8 nM NaHCO₃ vitamins 100 μg/L vitamin B12 80 μg/L p-aminobenzoic acid 20 μg/L nicotinic acid 100 μg/L calcium pantothenate 300 μg/L pyridoxine hydrochloride 200 μg/L thiamine-HCl•2H₂O 50 μg/L alpha-lipoic acid Electron acceptor 1.0. g/L NaNO₃, Na₂ fumarate or Fe(III) Na EDTA The pH of the medium is adjusted to 7.5. Strain L3:3 is expected to show growth via nitrate reduction and turbidity increase under denitrifying conditions as does LH4:18.

Example 15 Anaerobic Growth of Strain L3:3 on Oil as the Sole Carbon Source

Strain L3:3 and Shewanella strain LH4:18 were studied and compared in their abilities for anaerobic growth on oil as the sole carbon source using different electron acceptors. Shewanella strain LH4:18 has been show to grow using nitrate as the electron acceptor in commonly owned and co-pending US 2009-0260803 A1. Shewanella strains L3:3 and LH4:18 were inoculated into 20 mL serum vials containing ˜10 mL SL10 minimal salts medium (Table 2), supplemented with one of the following electron acceptors: NaNO₃ (2000 ppm), Na₂ fumarate (3500 ppm), or Fe(III) Na EDTA (5000 ppm), and overlayed with 5.0 mL of autoclaved crude oil. LH4-18 samples were excluded from NaNO₃ test vials. The medium and crude oil had been deoxygenated by sparging these reagents with a mixture of carbon dioxide and nitrogen (20% and 80%, respectively) followed by autoclaving. All manipulations of bacteria were done in an anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.) (gas mixture: 5% hydrogen, 10% carbon dioxide and 85% nitrogen). Replicate test vials were set up per electron acceptor treatment by L3-3 inoculum. The cultures were incubated at ambient temperature for two weeks. Cell growth/titer of the test cultures were analyzed by MPNs.

L3:3 grew anaerobically in oil enrichments where crude oil was provided as the sole carbon source when either NaNO₃, Na₂ fumarate, or Fe (III) Na EDTA was provided as the electron acceptor. A table of growth results as analyzed by cell titers recorded as MPN log 10 is listed below in Table 6. Strain L3:3 grew anaerobically 3 logs to cell titers of ˜10⁵-10⁷ cells per mL from starting titers of ˜10³ cells per mL after two weeks incubation time. The change in cell numbers as a result of anaerobic growth on oil are listed as the log₁₀ of the MPN recorded for growth ±0.5 log. The growth of Shewanella strain L3:3 on the different electron acceptors was comparable to that of Shewanella strain LH4:18. Strain L3:3 grew anaerobically on oil using either NaNO₃, Na₂ fumarate, or Fe (III) Na EDTA as the electron acceptor. Cell titers are presented as the average of replicate test vials. Shewanella strain LH4:18 also grew on oil using fumarate or Fe (III) Na EDTA as electron acceptor. Its growth on oil using nitrate as an electron acceptor had been previously demonstrated in commonly owned and co-pending US 2009-0260803 A1. Both L3:3 and Shewanella strain LH4:18 grew ˜3 logs to titers of ˜10⁵-10⁷ cells per mL from starting titers of 10³ cells per mL anaerobically after two weeks incubation time.

TABLE 6 Anaerobic Growth on oil Delta MPN log10 Electron Acceptor Strain NaNO₃ Na₂ fumarate Fe(III) Na EDTA Shewanella strain 3.0 3.2 2.7 L3:3 Shewanella strain n.t. 4.7 2.2 LH4:18 .n.t. = not tested

Example 16 Determining the Temperature Limits for Growth of Strain L3:3

To determine the optimal temperature range as well as tolerances for Shewanella putrefaciens LH4:18 and Shewanella sp L3:3, these strains were grown at different test temperatures as given in Table 7.

Inoculums of Shewanella strains LH4:18 and L3:3 were grown overnight (16 to 18 hours) aerobically in LB medium with shaking at 30-35° C. These overnight cultures were grown to visible turbidity and relatively high levels of cell counts as measured by optical density. Aliquots from these starter cultures were then used to seed flasks of 10 mL sterile LB medium that had been pre-incubated at a specific test temperature overnight. Temperature test cultures were seeded at an optical density of approximately 0.1 as measured using a spectrophotometer and visible light, wavelength of 600 nm. This constituted a dilution of starter cultures approximating between a 1:50 and 1:100 dilution. Growth was then measured by tracking the turbidity or optical density of cultures over time. The resulting growth rates determined for strains LH4:18 and L3:3 obtained for the different test temperatures is expressed as doubling time, the time to double cell number, in units of hours; the smaller the number the faster the growth rate. At doubling times of <2 h these strains are presumed to compete successfully with background microbial populations in situ. Table 7 shows the results for growth rates at the recorded temperatures. Both Shewanella strains were shown to grow at a rate that would allow them to compete with microbial populations in situ for a relatively broad range of environmental temperatures.

TABLE 7 Average Recorded Doubling Time for selected temperatures ° C. Doubling times (in hours) Temperature strain 10° C. 16° C. 22° C. 27° C. 30° C. 32° C. 35° C. 37° C. 41° C. LH4:18 3.18 1.71 1.02 0.95 0.87 0.79* 0.97 1.45 No growth L3:3 n.t. n.t. n.t. n.t. n.t. n.t. n.t. 0.98 0.63 n.t. = not tested

Example 17 Anaerobic Growth of Strain L3:3 in the Presence of Oil Under Dentrifying Conditions

To demonstrate the ability to grow anaerobically in the presence of oil under denitrifying conditions, an aliquot (10⁴-10⁵ cells) of each of Shewanella strains LH4:18 and L3:3 was inoculated under anaerobic conditions into 20 mL serum vials containing a 1:2 ratio of minimal salts medium supplemented with sodium lactate. The media formulation used was designed to promote growth and propagation of Shewanella strain L3:3 as well as the oil release mechanism within a reservoir environment. The medium composition for anaerobic growth was as follows: 10 mL minimal salts medium (Table 4 minimal salts medium), 1000 ppm sodium lactate and ˜2000 ppm sodium nitrate with 5.0 mL of autoclaved crude oil. Strain LH4:18 acted as a positive control for anaerobic growth under denitrifying conditions containing surface active agent(s). Both the medium and crude oil were deoxygenated by sparging the filled vials with a mixture of nitrogen and carbon dioxide followed by autoclaving. All manipulations of bacteria were done in an anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.). These cultures were incubated at ambient temperatures for several days and monitored for nitrate and nitrite levels, for visible turbidity, and for visible changes to the integrity of the oil phase.

Table 8 shows the results of this growth study in the presence of oil. A pure culture of strain L3:3 showed growth through a reduction in lactate and nitrate levels when grown in the presence of oil. These strains also showed ˜two to three logs growth as indicated by MPN data (Table 8).

TABLE 8 Nitrate Reduction as a Measure of Anaerobic Growth In the presence of Oil with lactate as the primary carbon source % % nitrate Lactate Bacteria 16S Genus reduction reduction MPN time isolate ID in oil in oil log10 (days) NIC¹ n.a. 8% 0% n.t.² 14 L3:3 Shewanella 58% 44% 7.0 14 chilikensis, JC5T LH4:18 Shewanella 51% 35% 6.4 14 putrefaciens ¹NIC: Non inoculated control ²n.t.: not tested

Example 18 Identification of Electron Acceptors which Promote Oil Release By Strain L3:3

Different terminal electron acceptors (shown in Table 9) were tested in anaerobic growth of strain L3:3 to determine its ability to grow on a range of terminal electron acceptors including fumarate as well as various metal oxides. A mixed culture of LH4:18 and L3:3 was also tested with nitrate and fumarate. Anaerobic test growths were set up using minimal salts media (Table 4). 20 mL of minimal salts medium was supplemented with 1000 ppm sodium lactate, where 2000 ppm sodium nitrate was used as the electron acceptor control. The milli-equivalents of the following electron acceptors were each applied in their respective electron assay sample: fumarate, pyruvate, Fe (III) sodium EDTA, manganese dioxide, and vanadium dioxide. The minimal salts base medium, lactate, and terminal electron acceptor preparations were all deoxygenated by sparging with a mixture of nitrogen and carbon dioxide followed by autoclaving. All manipulations of bacteria were done in an anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.). These cultures were incubated at ambient temperature for several days and monitored for growth by increases in visible turbidity as measured by OD/MPN or by lactate depletion as measured by IC. Results are shown in Table 9.

TABLE 9 Relative Growth obtained for Strains L3:3 and LH4:18 on different electron acceptors using Lactate as supplemental Carbon Source Iron Man- (Fe(III)) ganese Vanadium Nitrate Fumarate EDTA Dioxide Dioxide Pyruvate L3:3 + ++ ++ ++ + ++ L3:3 + + ++ n.t.¹ n.t. n.t. n.t. LH4:18 ¹n.t. not tested

Example 19 Strain L3:3 Increases the Contact Angle of Oil on Deep Sediment Sand

Strain L3:3 was grown aerobically overnight in SIB (Synthetic Injection Brine; Table 10) plus 1% peptone. Samples were then added into an anaerobic LOOS test, described above, and were supplemented with 1000 ppm sodium lactate and 2000 ppm sodium nitrate. After approximately one week, an aliquot of the sand was removed from the bottom of the strain L3:3 well and was visualized microscopically. FIG. 17(A) is a typical image of untreated oil coated sand. As indicated, the contact angle (qCA FIG. 17B) between the hydrocarbon and sand is low—the surface energy encourages the hydrocarbon to coat the entire mineral grain. FIG. 17(C) shows the effect of exposure of oil coated sand to strain L3:3. The contact angle (qCB-FIG. 17D) is increased dramatically indicating a significant change in the surface energy between the hydrocarbon and the mineral.

TABLE 10 Components of SIB1 Minimal Medium (per Liter) and added electron acceptor and electron donor NaHCO3 0.138 g CaCl2*6H₂O 0.39 g MgCl2*6H₂O 0.220 g KCl 0.090 g NaCl 11.60 g Trace metals (Table 4) 1 mL Vitamins (Table 4) 1 mL Na₂HPO₄ 0.015 g (10 ppm PO₄) NH₄Cl 0.029 g (10 ppm NH₄) Electron donor added Na-Lactate 0.124 g (124 ppm Na- Lactate) Electron acceptor added Na₂nitrate 0.4 g/400 ppm Adjust pH with HCl or NaOH Filter sterilize

Example 20 Demonstration of Strain L3:3 Oil Release Sandpack or Core Flood Assay

To test the amount of residual oil left in a sandpack after the oil soaked sandpack was flooded with a water solution that simulated the injection brine used in flooding an underground oil reservoir, the sandpack was fabricated as per standard methods described by Petroleum Reservoir Rock and Fluid Properties, Abhijit Y. Dandehar, CRC Press (2006). A similar core flood/sandpack apparatus and techniques used to operate it are also described by Berry et al. (SPE paper number 200056, SPE Reservoir Engineering, November 1991, p 429). The use of a similar apparatus and techniques for testing microbial treatments in a sandpack is described by Saikrishna et al. (SPE paper number 89473, (2004)).

To demonstrate that strain L3:3 is capable of oil release, a L3:3 culture was applied to a sandpack saturated with oil in an in-house developed Teflon® shrink-wrapped sandpack apparatus that simulates packed sand of sandstone. The process described herein was used for making two column sets, a “control” set and a “test” set, which was inoculated with L3:3 to test its efficacy to release oil from the sand column. Using a 1.1 inches (2.8 cm) thick, and 7 inches (17.8 cm) long Teflon heat shrink tube, an aluminum inlet fitting with Viton® O-ring was attached to one end of the tube using a heat gun. Alaskan North Slope sand was added to the column which was vibrated with an engraver to pack down the sand and release trapped air. A second aluminum inlet fitting with Viton® O-ring was attached to the other end of the tube and sealed with a heat gun. The sandpack was then put in an oven at 275° C. for 7 min to evenly heat and shrink the wrap. The sandpack was removed and allowed to cool to room temperature. A second Teflon® heat shrink tube was installed over the original pack and heated in the oven as described above. After the column had cooled, a hose clamp was attached on the pack on the outer wrap over the O-ring and then tightened. For this demonstration there were four sandpack columns assembled.

The four sandpack columns were flooded horizontally with three pore volumes of SIB1 Synthetic Injection Brine (Table 10) at 10 mL/min via a syringe pump and a 60 mL (BD) sterile plastic polypropylene syringe. All four sandpacks were then flooded with two pore volumes of anaerobic autoclaved crude oil at 0.5 mL/min to achieve irreducible water saturation. The crude oil was aged on the sand for three weeks prior to being inoculated with strain L3:3.

For inoculation, the culture was grown aerobically overnight in PPGAS media (Table 11). The culture was then placed in an anaerobic environment where sodium lactate was added to SIB1 minimal brine solution to a concentration of 1000 ppm and sodium nitrate was added to a concentration of 2000 ppm. The inoculation sample was then anaerobically aged in an anaerobic chamber (Coy Laboratories Products, Inc., Grass Lake, Mich.) for 5 days before inoculating the sandpacks. After the aging period, two columns were anaerobically inoculated with a sample of Shewanella sp L3:3 for one pore volume at 0.4 mL/hr. Two control sandpacks were flooded using anaerobic SIB1, using the same inoculation procedure. The four sandpacks were then shut-in for incubation with the oil for five days. After the shut-in, the columns were then produced for three pore volumes with anaerobic sterile SIB1 low bicarbonate at 0.4 mL/hr.

TABLE 11 Components for PPGAS Growth Medium (per Liter) Peptone   10 g MgSO₄  0.2 g KCl  1.5 g NH₄CL 1.07 g Tris HCL Buffer,  120 mL pH 7.5

At the conclusion of the production flood, the 7 inches long slim tubes were sacrificed into three 1.9-inch sections labeled A-C. One inch was skipped at the beginning and at the exit of the slim tube to avoid edge effects during analysis. Section “A” came from the front end of the column. Sections A, B and C were analyzed for residual oil saturation on the sand. The amount of oil on the wet sand from the sacrificed slim tubes for residual oil was measured by GC as described above. This value was multiplied by the total amount of toluene used to extract the oil resulting in the total amount of oil on the sand. The value obtained was then divided by the total sample weight to yield the percent of oil with respect to the total sample weight. The weight percent of oil of the sample was then multiplied by the ratio of the empirically derived characteristic of packed North Slope sand (total weight of sample after being flooded with brine divided by total sand weight, 1.27). This relationship is equal to the amount of oil on dry sand. This value was then multiplied by the ratio of the weight of the North Slope sand to the weight of the fluid trapped in the pore space of the sand, 3.75. The resulting value reflected the residual oil left on the sand in units of g of oil/g of total fluid in the pore space. As shown in Table 12, residual oil left on the column, in fractions A and C of the test column, were less than the controls confirming that the columns inoculated with the Shewanella sp. L3:3 released more oil than uninoculated control columns, with an average of 4.1% decrease in residual oil remaining on the columns when L3:3 was inoculated on the columns.

TABLE 12 Residual oil left on sand along the tube length after flooding with anaerobic sterile “Brine” Average Percent Column Residual Oil on Fraction Sand Assay Column A C Average. Test columns 12.6% 15.3% 13.9% Control 18.9% 17.1% 18.0% columns 

What is claimed is:
 1. A method for altering the wettability of a hydrocarbon coated surface comprising: a) providing a hydrocarbon-coated surface; b) providing a medium selected from the group consisting of: i) a cell containing medium comprising one or more isolated Shewanella sp.; and ii) a conditioned medium which is substantially cell free and which has been in contact with one or more isolated Shewanella sp.; wherein the Shewanella sp. comprise a 16S rDNA having at least 99% identity to the 16S rDNA sequence of SEQ ID NO: 3; c) contacting said hydrocarbon-coated surface with the medium of b) by a process comprising pumping water comprising the medium into a subsurface, wherein the medium alters the wettability of said hydrocarbon-coated surface.
 2. The method of claim 1, wherein the hydrocarbon-coated surface is a component of a terrestrial surface formation or subsurface formation comprising elements selected from the group consisting of rock, soil, brine, sand, shale, clays and mixtures thereof.
 3. The method of claim 2, wherein said hydrocarbon coated surface is contacted with the medium in either a producer well, an injector well or an environmental site.
 4. The method of claim 1 wherein the hydrocarbon coated surface is contacted with the medium by a process comprising; pumping water comprising the medium into a subsurface formation and allowing that water to be produced along with hydrocarbon at a producer well.
 5. The method of claim 3 wherein the hydrocarbon coated surface is contacted with the medium by a process comprising: pumping water comprising the medium into a subsurface formation down the producer well and then back-flowing hydrocarbon and water out of the producer well.
 6. The method of claim 3 wherein the hydrocarbon coated surface is contacted with the medium by a process comprising; a) inoculating an injector well with the medium wherein the injector well is in communication with one or more producer wells; and b) providing injection water that has been augmented with nutrients either continuously or periodically to the injector well; wherein oil is recovered at the producer well.
 7. The method of claim 3 wherein the hydrocarbon coated surface is contacted with the medium by a process comprising: a) pumping the medium comprising water onto an environmental site comprising a hydrocarbon coated surface wherein the hydrocarbon is released from the site; b) collecting the water and released hydrocarbon of (a); c) separating the hydrocarbon from the water; and d) recycling the water back to the environmental site wherein the water is combined with or treated with Shewanella sp. to produced medium.
 8. The method of claim 1 wherein the Shewanella sp. comprise a 16S rDNA comprising a degenerate signature sequence selected from the group consisting of SEQ ID NO: 19, SEQ ID NO:21 and SEQ ID NO:23.
 9. The method of claim 1 wherein the Shewanella sp. is a microorganism having the following characteristics: a) a 16S rDNA comprising signature sequences SEQ ID NOs: 13 and 14; and b) a riboprint pattern identifier of 212-824-S-4 as illustrated in FIG.
 16. 10. The method of claim 9 wherein the Shewanella sp is L3:3 (ATCC No. PTA-10980).
 11. The method of claim 1, wherein the medium comprises one or more additional microorganisms.
 12. The method of claim 1, wherein the medium further comprises nutrients for promoting growth of the Shewanella.
 13. The method of claim 12, wherein the nutrients are selected from the group consisting of peptone, yeast extract, and casamino acids.
 14. The method of claim 1 wherein the one or more Shewanella species produces a wetting agent.
 15. The method of claim 14, wherein the wetting agent functions to alter the wettability of said hydrocarbon-coated surface.
 16. The method of claim 1 wherein the alteration in wettability of step (c) promotes enhanced oil recovery.
 17. The method of claim 1 wherein the alteration in wettability of step (c) improves methods for bioremediation.
 18. A method for oil recovery from an oil reservoir comprising: a) providing one or more Shewanella sp; b) injecting an oil reservoir with the one or more Shewanella sp of (a); and c) injecting said oil reservoir with a nutrient solution comprising one or more electron acceptors selected from the group consisting of nitrate, fumarate, ferric ion, manganese (MnIV) ion and mixtures thereof; wherein said one or more Shewanella sp. grow under anaerobic conditions in the oil reservoir and said growth promotes improved oil recovery; and wherein the Shewanella sp. comprise a 16S rDNA having at least 99% identity to the 16S rDNA sequence of SEQ ID NO:
 3. 19. The method of claim 18 wherein injecting of (b) and (c) are simultaneous.
 20. The method of claim 18 wherein the one or more Shewanella sp. and the nutrient solution are mixed and injected together.
 21. The method of claim 18 wherein the Shewanella sp have the following characteristics: a) a 16S rDNA comprising signature sequences SEQ ID NOs: 13 and 14; and b) a riboprint pattern identifier of 212-824-S-4 as illustrated in FIG.
 16. 22. The method of claim 18 wherein the Shewanella is selected from the group consisting of L3:3 (ATCC No. PTA-10980).
 23. The method of claim 18 wherein the nutrient solution comprises at least one carbon source.
 24. The method of claim 18 comprising injecting the oil reservoir with one or more additional microorganisms.
 25. The method of claim 11 or claim 24 wherein the one or more additional microorganisms are selected from the group consisting of bacterial isolate Pseudomonas stutzeri LH4:15 (ATCC No. PTA-8823), Thauera sp AL9:8, (ATCC No. PTA-9497), and mixtures thereof. 